Scientifica

Volume 2013 (2013), Article ID 459405, 29 pages

http://dx.doi.org/10.1155/2013/459405

Review Article

Laboratory Diagnosis of Invasive Aspergillosis: From Diagnosis to Prediction of Outcome

Richard C. Barton

Mycology Reference Centre, Department of Microbiology, Leeds Teaching Hospitals Trust, Leeds LS1 3EX, UK

Received 15 October 2012; Accepted 14 November 2012

Academic Editors: J. R. Blazquez, G. Comi, and C.-Y. Hung

Copyright © 2013 Richard C. Barton. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

Invasive aspergillosis (IA), an infection caused by fungi in the genus Aspergillus, is seen in patients with immunological deficits, particularly acute leukaemia and stem cell transplantation, and has been associated with high rates of mortality in previous years. Diagnosing IA has long been problematic owing to the inability to culture the main causal agent A. fumigatus from blood. Microscopic examination and culture of respiratory tract specimens have lacked sensitivity, and biopsy tissue for histopathological examination is rarely obtainable. Thus, for many years there has been a great interest in nonculture-based techniques such as the detection of galactomannan, β-D-glucan, and DNA by PCR-based methods. Recent meta-analyses suggest that these approaches have broadly similar performance parameters in terms of sensitivity and specificity to diagnose IA. Improvements have been made in our understanding of the limitations of antigen assays and the standardisation of PCR-based DNA detection. Thus, in more recent years, the debate has focussed on how these assays can be incorporated into diagnostic strategies to maximise improvements in outcome whilst limiting unnecessary use of antifungal therapy. Furthermore, there is a current interest in applying these tests to monitor the effectiveness of therapy after diagnosis and predict clinical outcomes. The search for improved markers for the early and sensitive diagnosis of IA continues to be a challenge.

1. Introduction

Aspergillosis, which can be defined as an infection or disease caused by fungi in the genus Aspergillus constitutes a wide range of disease entities that form a continuum from allergic reactions to disseminated invasive disease in immunocompromised patients [1]. The specific term invasive aspergillosis (IA), often defined in relation to the primary affected organ as invasive pulmonary aspergillosis (IPA) is commonly considered to be defined by invasion of the pulmonary parenchyma by the growing hyphae of Aspergillus [2] and this is further refined being angioinvasive IPA if there is evidence of vascular invasion by the hyphae [2]. The most common aetiological agent of IA, Aspergillus fumigatus, is a ubiquitous fungus (Figure 1), with airborne conidia leading to almost universal and constant exposure in almost all humans. The corollary of this is that as the risk of IA is mainly a function of deficits in host defences, IA is seen primarily in patients with haematological malignancy and in solid organ and stem cell transplant recipients [3]. Diagnosis of IA is complicated by the fact that unlike many infections blood culture is almost always negative for A. fumigatus [4] and sampling of the lower respiratory tract by bronchoalveolar lavage in order to culture the fungus is also insensitive [5]. This lack of diagnostic tools has led to an explosion in the development and evaluation of nonculture diagnostic approaches including imaging, PCR-based detection of Aspergillus DNA, and antigen detection—particularly the detection of galactomannan in serum and bronchoalveolar lavage [6]. The difficulties in making a diagnosis of IA lead initially to considerable variation in how cases were defined [7]; however, in more recent years, criteria for the identification of IA have greatly benefited from the European Organisation for the Research and Treatment of Cancer (EORTC) and US Mycoses Study Group (MSG) criteria for defining invasive fungal infections including IA [8, 9]. Though it has been noted that whilst these criteria have been readily taken up, lack of compliance with them even in studies purporting to use them as reference standards continues to hamper comparisons of diagnostic investigations [10]. Nouer et al. [11] have suggested a modified version of these criteria specifically for IA. Together with the development of improved diagnosis of IA, there has been a steady increase in the numbers of licenced antifungals effective against IA [12]. This has resulted in an overall significant improvement in outcomes of patients with IA [13, 14]; however, this has been effected in part through the extensive use of empiric antifungal therapy [15]. The challenge for the current day is to identify diagnostic strategies that reliably detect or predict IA in order to target therapy and improve outcomes or sustain existing outcomes without the need for unnecessary empiric therapy.

Figure 1: A. fumigatus (bar is 10 um).

1.1. Site of Disease

IA is predominantly a disease of the respiratory tract in most cases involving the lung parenchyma [2] but the disease may also involve the pleura and the trachea and bronchi [16]. From these sites, dissemination is reported to occur from pulmonary sites in 10%–25% of cases, particularly to the brain and also including liver, kidney, gut [17], and skin [18]. The sinuses are also an important site for aspergillosis [19] and there has been a recent review drawing attention to skull osteomyelitis following invasive otitis externa [20].

1.2. Aetiology of Disease

The most common cause of all forms of IA is A. fumigatus. This is one of the most common species in the environment and this fact together with its small spores provides greater penetration to the small airways and ability to grow at 37°C account for its predominance as causal agent [21]. A. flavus is the second most common causal agent followed by A. niger [22]. However, cases caused by A. terreus are seen commonly in some centres [23, 24]. A. flavus is frequently seen in nonpulmonary diseases and in developing countries [25, 26]. A new species, A. tanneri, that causes invasive disease in patients with chronic granulomatous disease has recently been described [27]. There has been a recent recognition that amongst isolates of some species of Aspergillus there are in fact mixtures including cryptic species that can often only be distinguished by DNA sequence analysis. Within isolates thought to be A. fumigatus, species such as A. lentulus, A. novofumigatus, and A. fumigatiaffinis and the teleomorphic species Neosartorya udagawae have been found upon close examination [28, 29]. Species such as A. tubingensis and A. awamori have been found amongst clinical isolates previously identified as A. niger [30]. These distinctions may seem as taxonomic niceties but these newly recognised species are often associated with distinct patterns of susceptibility to antifungals (Table 1) [30, 31].

Table 1: Antifungal susceptibilities for different species of Aspergillus.

Species
Resistance to
Frequency

A. fumigatus
Itraconazole
Occasional, increasing

Voriconazole
Rare, increasing?

Posaconazole
Rare, increasing?

Echinocandins
Rare

A. lentulus
Amphotericin B
Intrinsic?

Itraconazole
Intrinsic?

Voriconazole
Intrinsic?

A. fumigatiaffinis
Amphotericin B
Intrinsic?

Itraconazole
Intrinsic?

Voriconazole
Intrinsic?

A. terreus
Amphotericin B
Intrinsic

A. flavus
Amphotericin B
rare

Itraconazole
rare

Voriconazole
rare

A. niger
Itraconazole
Occasional

A. awamori
Itraconazole
Occasional

A. tubingensis
Itraconazole
Intrinsic?

A. acidus
Itraconazole
Intrinsic?

1.3. Epidemiology of Disease

IA has traditionally been a disease associated with patients with reduced levels of neutrophils, an observation made in the early 1970s [32] together with the finding that neutrophils were capable of the killing of Aspergillus hyphae in vitro [33]. Thus, IA has mainly been reported as a disease of patients with neutrophil deficits resulting from myeloablative chemotherapy for haematological malignancy and as part of conditioning for stem-cell transplantation [34–37]. While often grouped together for analysis, SCT and acute leukaemia patients may actually present with distinct forms of IA with consequences for optimal diagnostic approaches [38]. The incidence of IA in haematological malignancy varies markedly from 1.7% in a recent study from Italy [39] to nearly 30% in a Dutch study [40] and will be affected by intrinsic factors including recently recognised genetic predisposition to aspergillosis together with the use of antifungal prophylaxis and the extent to which systemic diagnostic screening is performed. Solid organ transplantation, particularly lung and liver transplant, also poses a significant risk for IA [41–44]. Corticosteroid use, particularly during SCT has been recognised as an important risk factor for IA [45]. In recent years, groups of nonneutropenic patients have been shown to at increased risk of IA [46, 47] including patients with chronic obstructive pulmonary disease (COPD) [48], severe liver disease [49], patients in intensive or critical care [50, 51], patients suffering from influenza with H1N1 virus [52], and following surgery [53]. Patients with HIV/AIDS are typically at low risk of IA as immune defect is in CD4 cells which do not appear to play an important role in combating aspergillosis; however, cases of IA in AIDS have been reported [54]. Patients with chronic granulomatous disease (CGD) are at risk of a peculiar form of IA often presenting as fulminant pneumonitis [55]. Genetic factors affecting susceptibility to IA are beginning to be understood and examined. People with a mannose-binding lectin deficiency and mutations in some Toll-like receptors are likely to be at higher risk of IA [56, 57].

1.4. Outcomes in IA

The consequences of the development of IA in patients improved markedly in the last 20 years. In 1990, Denning and Stevens surmised that mortality from IA in SCT was greater than 94% [58]. In 2009, results of a prospective antifungal therapy (PATH) registry study indicated that 12-week mortality of patients with HSCT was 35% [14]. A European study of patients with haematological malignancy showed that 12-week mortality was 42% and had declined over the period of the study between 2004 and 2009 [59]. A study of pediatric patients with IA reported a 3-year survival of 55% [60]. However, succumbing to IA remains a factor decreasing the short- and long-term chance of survival. In a study of patients with acute myeloid leukaemia having IA reduced chances of survival at 2-years from 32% to 14% [61]. Analysis of hospital discharge and other medical data in the US has shown that, in general, IA is associated with significantly higher levels of mortality, hospital costs, and length of stay [62–64] compared to similar patients without IA.

1.5. Diagnosis of IA

The signs and symptoms of IA are generally nonspecific, and typically involve failure to respond to antibacterial therapy given empirically for fever. Biochemical markers of inflammation such as C-reactive protein or procalcitonin are also nonspecific, though they may have value in monitoring the success of treatment once a diagnosis is established [65, 66]. Approaches to making a specific diagnosis IA can be categorised as involving: imaging, direct microscopy, histopathology, culture, antigen detection, and DNA detection (Table 2).

Table 2: Main approaches to laboratory diagnosis.

Test
Specimens
Advantages
Disadvantages

Direct microscopy
Respiratory
Low cost
Insensitive, labour intensive

Culture
Respiratory, tissue
Low cost, enables further analysis
Insensitive

Histopathology
Tissue
Enables proven diagnosis
Requires biopsy tissue

Galactomannan (GM)
Serum, BAL
Sensitive, specimens easy to obtain
Lacks sensitivity in patients on antifungals

β-D-glucan (BDG)
Serum
Sensitive, specimens easy to obtain
Lacks specificity

PCR (DNA detection)
Any
Sensitive, can be applied to any specimen
Labour intensive, expensive

Since the work of Caillot et al. in 2001 showed both the specificity and limitations of the high resolution computerised tomography (HRCT) scan of the chest with the signs of the halo and later the air crescent, HRCT has formed an essential investigation of all patients suspected of having IA [67]. Importantly, the halo sign has been recognised as specifically linked to angioinvasive IA [68]. Other signs such as “tree in bud” and segmental consolidation have been recognised as associated with airways disease as compared to angioinvasive aspergillosis [69]. However, studies of 70 patients with IA or pulmonary lymphoma highlighted the difficulties in relying purely on CT imaging to diagnose IA where no single feature provided sufficient sensitivity or specificity [70], and a study of the HRCT signs produced by IA, candidiasis, and cryptococcosis showed a lack of specificity of the halo or air crescent signs for IA [71]. 68Ga-labelled iron siderophores visualised in positron emission tomography (PET) showed promise in rat model of IA as a potential specific imaging technique [72]. This paper will focus on laboratory markers of IA.

One of the problems faced with any disease, where markers have been used to define cases of a disease, is how to make comparisons with newer markers. This has been particularly problematic with IA and has for example restricted the analysis of the galactomannan (GM) test applied to serum where it is often used to define probable IA. It has, for example, only been possible to analyse the value of bronchoalveolar lavage (BAL) GM results in the smaller number of patients who have proven IA where disease is defined by the presence of fungal hyphae and culture in tissue biopsy material [73].

2. Direct Microscopy

One of the simplest approaches to diagnose IA is to examine appropriate specimens microscopically. However, this approach is inherently lacking in specificity as Aspergillus sp. rarely sporulate in vivo and hyphae seen may represent any number of filamentous fungi. The reported sensitivity of this approach is quite variable from 0% to 90% [74–76] which may reflect differences in detailed methodology such as use of calcoflour (Figure 2) [77].

Figure 2: Calcoflour stained tissue from a wound infection that grew A. flavus. Bar = 10 um.

3. Histopathology

Demonstrating tissue invasion by a filamentous fungus through histopathological examination of biopsy or autopsy material provides a diagnosis of proven invasive fungal infection (IFI) [78]. Since it is not usually possible to identify a fungus from mycelium seen in tissue sections, positive culture of Aspergillus from the same specimen is required to make a proven diagnosis of IA. The value of proven IA is high but in most cases obtaining biopsy samples, in the case of pulmonary IA by transthoracic biopsy is often contraindicated due to low platelet counts or other medical risk. In one case series, only 2/5 patients sampled by transbronchial biopsy were found to have hyphal invasion of the tissue sample, the other 3 were diagnosed as having probable IA based on positive serum and/or BAL GM [79]. Careful examination of tissue sections by standard haematoxylin and eosin staining should reveal the presence of Aspergillus hyphae but stains such as period acid Schiff and Grocott’s silver may add sensitivity and should be carried out whenever a fungal infection is suspected (Figure 3) [80]. Aspergillus hyphae seen in tissue sections tend to be narrow (1–3 um in diameter) and septate and cannot easily be distinguished from a number other fungies that cause infections including Fusarium and Scedosporium. It is usually easy to distinguish Aspergillus hyphae from the wider and pauciseptate hyphae of the mucoraceous moulds such as Rhizopus and Lichtheimia sp. (histPath book). Some authors have reported methods of identifying fungal cells in fixed tissue sections by immunohistochemical labelling [81]. These techniques are technically demanding and together with the fact that the clinical material to apply these methods is likely to be infrequently sent for investigation means that these methods are unlikely to become popular. PCR identification of hyphae seen in fixed tissue specimens may be able to provide a method of identification if culture of the tissue specimen has not been performed [82].

Figure 3: Grocott’s silver stained infected lung tissue showing the black hyphae of Aspergillus invading lung tissue that is counterstained blue-green. Bar = 10 um.

4. Culture

Obtaining a positive culture of Aspergillus from a clinical specimen is a traditional way of making or contributing to the making of a diagnosis and prior to the use of GM and PCR was the main specific laboratory investigation for IA [83]. A positive culture will also enable other forms of analysis such as susceptibility testing. In technical terms, most Aspergillus sp. grow relatively rapidly (typically within 48 hr) and on most microbiology media including both mycological media such as Sabouraud’s agar and blood agars used for general bacteriological culture. Mortensen et al. claim to be able to increase the number of positive cultures by 17% by extending incubation time from 2 to 5 days [84]. While the technique of culturing specimens is inherently simple and low cost, an enhanced method of sensitively, rapidly, and specifically detecting digitonin immobilised microcolonies of Aspergillus using the enzymatic cleavage of a fluorescent compound has been described [85].

Identification of cultures of most species Aspergillus is generally straightforward [De Hoog atlas] by colony and microscopic morphology, though atypical forms, for example, A. fumigatus, have been known for many years [86]. More recently, atypical forms of A. fumigatus have been re-identified as new species including A. lentulus, A. novofumigatus, and A. fumigatiaffinis and these require DNA sequence analysis to be reliably identified [28, 29].

Using the EORTC criteria, in host and clinical (imaging) factors, positive cultures of Aspergillus from respiratory specimens are assumed to represent infecting fungus [87, 88]. In patients where a positive culture is not supported by both host and clinical factors, such cultures are typically interpreted as colonisation [89, 90]. The main problems described for the culture of respiratory and other specimens for the diagnosis of IA are the lack of sensitivity and the difficulty in distinguishing between infection and colonisation. The percentage of neutropenic patients diagnosed with IA by GM positive BAL who are positive by culture ranges from 10% to 58% [91–100]. In a study of the performance of a PCR and the GM assay on BAL samples mostly from haematology patients, in 17 cases of proven or probable disease where the mycological component of the diagnosis was by serum GM, only 7 were culture positive [101]. Failure to culture Aspergillus from respiratory specimens may lead to the incorrect assignment of Candida sp. as the aetiological agent from positive cultures and this may have led to the suggestion that HRCT signs previously thought of as pathognomic for IA are being also attributed, probably erroneously to invasive candidosis [102]. In a rabbit model of IA, culture of BAL varied in sensitivity in untreated animals from 50% to 100% depending on the infecting Aspergillus sp. [103]. A. fumigatus infected rabbits treated with amphotericin B became completely culture negative whilst signal was still obtained from GM or PCR testing of BAL, indicating the advantage of culture in terms of detecting viable fungus.

5. Galactomannan Detection

Galactomannan (GM) is a carbohydrate molecule composed of a backbone of mannose residues with side chains of β 1–5 linked galactofuranosyl residues. Detection of this molecule was described by Stynen in 1992 using a monoclonal antibody (EB-A2) [104] which specifically binds to four galactofuranosyl residues leading to the suggestion that GM, as detected by EB-A2 in the diagnostic ELISA which was later developed, is better referred to as galactofuranose [105], though this terminology has not been widely adopted. Pure GM is readily released from Aspergillus sp. growing in vitro as a molecule of about 20 kDa in size, but it is also present in larger molecules linked to proteins as glycoproteins [106, 107] and a lipopeptide galactomannan [108]. GM is part of the cell wall along with chitin, β 1–3, and 1–4 glucan [109], and while the GM is likely to be incorporated during periods of logarithmic growth this is also the stage of growth in vivo at which GM release peaks [110, 111] presumably because of leakiness in the hyphal tip during active growth. The extent to which active logarithmic growth occurs during infection in vivo is unclear but may be restricted by lack of nutrients particularly in necrotic tissue. The release of GM glycoproteins is thought only to occur during cell wall lysis which may occur in vivo where nutrients are limited and growth also is restricted by the host response and in necrotic oxygen deprived tissue [112]. The level of EB-A2 positive material during growth in vivo also appears to relate to the secretion of beta-galactofuranosidase which degrades the galactofuranosyl epitopes of this antibody [113, 114]. From an elegant in vitro model of the invasion of lung tissue where the release of various components in alveolar and endothelial compartments can be detected, it has been suggested that GM is not released into the circulation during infection until the fungus invades the endothelial compartment [115]. This suggests that circulating GM cannot be detected until angioinvasion by the fungus occurs. Release of GM into the circulation during angioinvasion is supported by the observation that serum GM is almost always readily detected in neutropenic haematological and SCT patients where angioinvasion is seen in characteristic halo signs in HRCT [116]. In contrast, in patients with chronic granulomatous disease, IA is often characterised by lung abscess development which may limit angioinvasion and patients are frequently serum GM negative [117]. Once in the circulation, levels of detectable GM are likely to be subject to clearance through the kidneys and by active uptake by macrophages [118]. Antibodies to GM can also develop which have been suggested as a cause of false negative serum GM results in patients with IA [119].

5.1. The GM Assay

The original assay for GM was a latex agglutination LA test with a limit of detection of 15 ng/mL, which was soon replaced by a sandwich ELISA able to detect less than 1 ng/mL [120], and most of the literature where the assay is used relates to the ELISA assay. The original specimens used in the GM assay were serum and urine. GM which can be detected in the urine of patients with IA [121, 122]. Animal models suggest that excretion of a significant proportion of GM occurs in the urine [118]. Early reports suggested that in human IA urine was a more sensitive specimen than serum [123], which was contradicted by the findings of others [124]. Furthermore, there is concern that GM is more likely to be detected in the urine of patients who are further down the course of invasive disease and where interventions are less effective [125]. The variety of methods used in these early studies, together with differences in pretreatments, mean that the value of urine as a specimen for GM detection remains unclear [126] and urine testing for GM is rarely used in recent studies. In contrast, the interest in BAL as a specimen for GM analysis has increased markedly since original observations of the presence of GM in BAL fluid [127] and BAL along with serum are currently the only specimens approved by the manufacturers for analysis. BAL is an attractive clinical material for analysis of pulmonary IA, as it has been shown that GM is released during hyphal growth rather than from conidia [128, 129] thus potentially enabling the distinction between colonisation and active infection. The difference between the yield of bronchial lavage (BL) as compared to BAL has been investigated and some have suggested that BL is more sensitive than BAL for the GM test, though conversely BAL was more sensitive for culture [130] though this has not been confirmed in subsequent studies [131]. A series of studies in patients with haematological malignancies and undergoing stem cell transplantation [91, 132–138], lung, and other solid organ transplant recipients [89, 99, 139] and patients in critical care [140, 141] have confirmed the value of BAL as a specimen for GM. GM has also been detected in lung abcess fluid [142]. More recently, it has been reported that detection of GM in sputum in cases of IA in haematological malignancy may prove useful [143]. Using a cutoff of 1.2 100% sensitivity and specificity for sputum was obtained compared to values in BAL of 62% and 83%, respectively, and this may prove a valuable less invasive sample to test. Cerebrospinal fluid (CSF) is another specimen type used for the detection of GM during attempts to diagnose central nervous system IA. The brain is the most common site for dissemination from the lungs. CSF may not be thought to be the most appropriate specimen for the diagnosis of central nervous system IA which tends to present as cerebral abscess and culture of CSF is rarely positive in cerebral IA [144]. However, GM has been detected in several cases of CNS IA [145]. In a study of 5 bone marrow transplantation patients with cerebral IA, the mean GM level in CSF was positive and higher than that in patients without IA [146].

In the commercial kit, there is a pretreatment step with an acid EDTA solution and heating in order to precipitate proteins and break up immune complexes. This may reduce the activity of the acid labile furanosyl side chains of GM and any galactofuranosyl moieties of glycoproteins may also be lost in this step [147]. It has been suggested that a microfiltration concentration step can be used to increase analytical and clinical sensitivity [148]. Some authors have described problems with the reproducibility of the assay [149]. Recently a monoclonal antibody that detects GM-like antigens was derived and used to develop a lateral flow assay to revisit the potential for diagnosing IA by detecting GM in urine [150].

5.2. Galactomannan Is Not Unique to Aspergillus sp.

GM is found in varying amounts in other fungies including Penicillium, Fusarium, Alternaria, and Histoplasma [151–153]. This presents a variety of problems. The ability to detect Penicillium marneffei, the only pathogenic Penicillium species, through GM detection is unlikely to result in clinical dilemmas since P. marneffei infections are seen in very distinct patient types compared to IA, that is, HIV with travel history to Southeast Asia [153]. On the other hand, cases of histoplasmosis seen in solid organ transplant recipients where serum and BAL specimens were positive for GM can create difficulties in patient management and these results are often referred to as false positives [154]. Similarly, patients with systemic Fusarium infection, seen classically in haematological malignancy, have also been found to be positive for the GM test though some authors take a more positive view in terms of the use of this assay for the diagnosis of Fusarium infection [155, 156]. Perhaps, most controversially, some authors have claimed that antigens from Cryptococcus neoformans cross-react in the commercial GM test and positive reactions seen in patients with cryptococcosis [157]. Positive results have also been reported for infections cause by other yeasts such as Geotrichum capitatum [158]. Swanink et al. who surveyed a range of fungi for cross-reacting antigens suggested that Candida sp. did react in the GM assay at a low level [159], and when sufficient numbers of yeast cells are processed, positive signals can result (R. Barton, unpublished data), a finding that have unlikely an impact on serum specimens but might result in false positives in BAL samples.

A more important problem resulting from the presence of cross-reacting antigens in Penicillium is the presence of GM in preparations of some antibiotic agents. False positives resulting from the use of piperacillin tazobactam have been reported since 2003 in patient sera and confirmed on testing antibiotic preparations [160, 161]. Recent investigations into the presence of GM in tazobactam from different manufacturers suggest that while there are still manufacturers whose antibiotic continues to be associated with false positive GM results [162], the problem has largely abated [163]. Other sources of false positive GM results include nutritional supplements [164, 165], and there have been theories of other foodstuffs including milk [166] and pasta [167] where cross-reacting antigens are thought to translocate from the gut to the blood and cause false positives, particularly in cases of gut mucosal disturbance during chemotherapy and in children. Most recently, galactomannan has been found in preparations of electrolyte solutions such as PlasmaLyte. Gluconate in some of these preparations is derived from A. niger, and GM from A. niger is present to the extent that it may cause false positive reactions [168–170].

One of the most carefully investigated cross-reacting antigens are those found associated with gut bacteria Bifidobacterium sp. Mennink-Kersten et al. hypothesised that lipoteichoic acids associated with the cell wall of Bifidobacterium sp. bind to the EB-2A monoclonal used in the GM ELISA [171] and that this was linked to the high rate of false positives seen in children and neonates. This was followed up by the demonstration of the cross-reactivity of almost all Bifidobacteria sp. tested in the GM assay and the presence of these bacteria extensively in neonatal faeces [172]. This theory was prompted by findings of the relatively poor specificity of the GM assay in neonates and children. Siemann et al. reported that in 5/6 premature neonatal patients aged between 19 and 136 days, sera were strongly positive for galactomannan, and in 3 cases sera tested positive repeatedly [173]. However, this is the only evidence for the problem of specificity in neonates, this is possibly because neonates are not a major at risk group for IA and are rarely tested. In general, specificity in slightly older paediatric patients is >90% [174–177].

5.3. Clinical Validity of GM Testing

A systematic review of serum GM testing for the diagnosis of IA was published in 2006 by Pfeiffer et al. [178]. Twenty-seven studies published between 1999 and 2005 were included and the main analysis was in patients with proven disease, defined by histological evidence of tissue invasion, reducing incorporation bias as the GM test itself can be used to define probable IA according to EORTC/MSG criteria [8, 179]. The overall sensitivity of the test for proven IA was determined to be 71% and specificity 89%. The limitation of this analysis was that at the time when most of the studies were published, a cutoff of 1.5 or 1.0 was being used and only 5 studies provided using this cutoff of 0.5, which is now recognised and used as a standard. In the studies, by using the 0.5 cutoff, ironically a sensitivity of 27% and overall the accuracy of the test improved with increasing the cutoff. Significant heterogeneity was observed amongst studies, particularly in sensitivity as had earlier been noted by Leeflang et al. [180] and attention was drawn to the lack of sensitivity in studies of patients with solid organ transplantation (22%). Importantly, there was little difference in the performance of the test between adults and paediatric patients.

In 2008, Leeflang et al. published a Cochrane review and meta-analysis of the GM assay on serum specimens including 30 studies between 1998 and 2007 [180] and included in analysis either proven or probable cases where the mycological criterion was defined by an alternative method to serum GM, for example, a positive BAL culture. Again, a minority of these studies, seven, used a cutoff of 0.5 and in this subset a sensitivity of 79% and specificity of 82% were obtained. It has been noted by other authors (Table 2) [181] that the incidence or pretest probability will affect the value of the GM (and any other test), particularly the positive predictive value. Leeflang et al. noted that at a prevalence of 8% of IA as seen in their meta-analysis, applying the test with a cutoff of 0.5 would lead to missing a diagnosis of IA 2% of patients and treating 17% of patients unnecessarily in a population of at-risk patients [180]. Again significant heterogeneity was seen though there were small numbers of patients with IA in some studies. A recent meta-analysis of 34 studies of the use of serum GM to diagnose IA between 1991 to 2008 suggested that the pooled sensitivity was as low as 66% and specificity was 90% [182]. Again significant heterogeneity was observed. At the incidence of IA observed of 10%, rates of under diagnosis and misdiagnosis were higher at 34% and 10%, respectively. Studies of the efficacy of serum GM to diagnose IA published more recently between 2009 and 2012 suggest that authors findings on the proportion of patients with IA that are positive for GM continues to vary ranging from 13% to 87.5%. The specificity of the assay on serum tends to be higher ranging from 21% to 100% and in most cases greater than 80%.

The most carefully analysed variable is the effect of mould-active antifungal therapy, typically for prophylaxis, on the sensitivity of the serum GM assay. Marr et al. analysed data for 317 immunocompromised patients finding overall sensitivity of the serum GM assay to be 70% for proven and probable IA, where the GM test itself was not used to define disease, and at a GM cutoff of 0.5 [186]. However, the sensitivity of the assay in patients receiving antifungal therapy (mostly itraconazole) on the day of diagnosis dropped to 52% compared to 89% in patients not receiving antifungal therapy. In other words, in this study, in patients on mould active antifungal therapy with breakthrough IA, serum GM was only effective in diagnosis in about half of the cases [187]. This result could be logical where antifungal treatment inhibits growth of Aspergillus or the cells renders nonviable reducing the load of fungal cells able to shed the GM antigen. Certainly animal models of IA have shown that the burden of Aspergillus as measured by lung chitin and galactomannan correlates with the level of circulating GM [188]. Similarly in vitro models of treatment appear to correlate reduction in fungal load with galactomannan [115]. The effect of the timing of the exposure of the antifungal exposure relative to the establishment of the inoculum is clearly critical. In the relatively unsophisticated model of Winn et al. where antifungal was added to germinating A. fumigatus conidia and GM release monitored, growth and GM levels were suppressed [189]. However, Hope et al. in their two compartment model, showed that delaying the amphotericin treatment of the same dose of the Aspergillus inoculum by six hours resulted in a failure to suppress GM release into the endothelial compartment which models the release of GM in the blood stream following pulmonary disease [115]. It has also been suggested that actively growing Aspergillus hyphae exposed to antifungals might increase the release of GM. Petraitiene et al. [190] described a rabbit model of IA treated with caspofungin where antifungal therapy resulted in an increase in GM despite improvements in terms of animal survival [190]. However, this increase in GM levels was again associated with increased fungal load, a function of the so-called paradoxical effect of echinocandin antifungals. However, in breakthrough cases of IA, perhaps due to resistance in Aspergillus or suboptimal drug levels during prophylaxis, where in order for a disease to become apparent, fungal burden must presumably increase, it remains to be seen how Aspergillus exposed to antifungal agents might result in infections where less GM is shed into the blood.

Another possible cause of the variability in sensitivity of the serum GM assay is the level and nature of immune suppression of the patient. Classically, the assay has been applied to patients with haematological malignancy or having undergone bone marrow or stem cell transplantation, both groups with low neutrophil counts. Cordonnier et al. have recently shown that amongst haematology patients with neutrophils levels /L are more likely to have higher serum GM levels than patients with higher neutrophil levels [191]. The serum GM assay has been shown to be modestly sensitive in COPD patients with IA [192, 193] and poorly sensitive in solid organ transplantation [194, 195] though more recent studies have achieved greater sensitivities in this patient group [196]. The lower incidence of neutropenia in these two patient groups may well account in part for the reduced sensitivity of the serum GM assay. Serum galactomannan was shown to have lower sensitivity in patients who had antibodies to Aspergillus fumigatus [119]. Finally, there are a number of laboratory parameters that will affect the probability that a patient is scored positive for a serum GM test including the frequency of testing, whether one or two positives are used to define a case of IA and the cutoff used. Some of the studies with the highest sensitivity have involved at least twice weekly sampling [197, 198]. There is a clear relationship between the cutoff used to define a positive score in the GM assay and the sensitivity. The original Bio-Rad Platelia assay recommended a cutoff index for positivity of 1.5, with indices of 1–1.5 considered an equivocal zone [199]. Currently, a cutoff of ≥0.5 is positive and <0.5 is negative. Meta-analysis showed that the sensitivities at 1.5, 1.0 and 0.5 cutoff are 62%, 71% and 79%, respectively [180]. A later meta-analysis [200] showed, unsurprisingly, that requiring two positive sera to define IA reduced sensitivity and increased specificity.

5.4. Clinical Validity of BAL GM

Guo et al. [184] have analysed the present considerable literature on the use of BAL as a specimen for the GM assay. Thirteen studies between 2003 and 2009 were considered and an overall sensitivity of 90% and specificity of 94% were calculated. A more recent meta-analysis of 30 studies gave figures that were slightly lower (87 and 89%, resp.) (Table 3) [201]. This sensitivity is notably higher than that seen in many studies of serum GM and the diagnostic odds ratio is notably higher than all blood-based tests. Analysis of 33 cases of IA where a blood sample and BAL specimen were taken within a week and where one or both were positive showed that all 33 BAL specimens had positive GM indices >0.5 compared to 9/33 (27%) of the sera [202]. Receiver operator characteristic (ROC) curve analysis of GM data from BAL and serum in a series of patients with proven or probable IA showed higher areas under the curve (AUC) for BAL testing compared to serum [141]. One of the observations that most studies note is that the background level of GM or EB-A2 positive material in BAL is greater than in serum [203]. This has raised the question of what is the appropriate cutoff for the assay applied to BAL material. The manufacturers of the kit, Bio-Rad, recommend the same cutoff as in serum, that is, >0.5 indicating a positive score [199]. However, values of 0.5 to 2 have been suggested [184]. Analysing the results of BAL GM testing in patients with haematologic disease showed that increasing the cutoff between 0.5 and 4 increased the positive likelihood ratio from 5 to 25 [204]. Using ROC curve analysis on 85 BAL GM data from paediatric patients at risk of IA, Desai et al. suggested that an optimum cutoff would be 0.87 giving a sensitivity of 78% and specificity of 100% [205], and a similar analysis leads Desai et al. [205] to propose a cutoff of 0.8. Park et al. 2010 [206] have even suggested using a cutoff of 0.2, and though applying this to a cohort of 359 at-risk patients gave a sensitivity and specificity of 86%, and 74%, respectively, a cutoff this low in a specimen that tends to have high background levels of GM is likely to lead to large numbers of false positives in most settings. Although the specificity of BAL GM testing is typically high, Acosta reported an intensive care patient with high levels of BAL GM without corroborating evidence of IA, direct microscopy and culture were negative, and who recovered without antifungal therapy [141]. Penicillium sp. colonisation may result in false positives [207, 208].

Table 3: Diagnostic accuracy of the main laboratory markers for IA.

Reference
Method
Sample
Sensitivitya
Specificitya
DORb

Mengoli et al. 2009 [183]
PCR (1)
Blood
0.88 (0.75–0.94)
0.75 (0.63–0.84)
22.11 (7.77–62.92)

Mengoli et al. 2009 [183]
PCR (2)
Blood
0.75 (0.54–0.88)
0.87 (0.79–0.93)
21.33 (6.86–46.63)

Leeflang et al. 2008 [180]
GM
Blood
0.79 (0.61–0.93)
0.82 (0.71–0.83)
17.10c

Sun et al. 2010 [182]
GM
Blood
0.66 (0.61–0.70)
0.9 (0.89–0.90)
19.1 (12.67–28.79)

Guo et al. 2010 [184]
GM
BAL
0.86 (0.70–0.94)
0.89 (0.85–0.92)
51.0c

Onishi et al. 2012 [185]
BDG
Blood
0.77 (0.71–0.82)
0.83 (0.82–0.84)
23.2 (9.9–54.4)

Sensitivity and specificity as proportions with 95% confidence intervals (CI) given in brackets, bDOR diagnostic odds ratio, ccalculated from sensitivity and specificity data in the references, 95% CI not calculable.

6. Detection of 1,3 β-D-Glucan (BDG)

The cell walls of Aspergillus contain relatively large amounts of glucan of which 1,3 -D-glucan forms a large part [209]. In vitro analysis of growing A. fumigatus showed that, like GM, BDG is released during logarithmic growth, though slightly later [210]. Unlike GM, BDG is widely distributed in the fungal kingdom and is found in the cell walls of many pathogenic fungi including Candida, Fusarium, and Pneumocystis though it is present at a lower level in Cryptococcus and virtually undetectable in the mucoraceous moulds [211]. Similar to GM, BDG is excreted into the culture fluid of A. fumigatus [212, 213].

6.1. The 1,3 β-D-Glucan (BDG) Assay

BDG can be detected through a pathway in the Limulus amoebocyte lysate (LAL) coagulation cascade that has traditionally be used for the detection of bacterial endotoxin. Whilst endotoxin interacts with LAL via factors B and C, factor G in the LAL interacts with BDG activating a proclotting enzyme which can then cleave a chromogenic substrate to generate a product detectable by spectrophotometry down to 10 pg/mL [214, 215]. Animal models of IA [216] and patients with IA [214, 217] were shown early on to have often high levels of BDG in serum validating BDG detection and as a potential diagnostic marker. Using pre-EORTC criteria of 30 definite or suspected pulmonary IA cases, 63% were positive by BDG using a cutoff of 20 pg/mL [218], and 73% of 185 control patients were negative. Patients with other fungal infections have been found to be positive for the BDG assay including those infected by Candida, Fusarium sp., Acremonium sp., Pneumocystis, and Histoplasma capsulatum [217, 219–221]. Thus, the BDG assay has emerged as a generic marker for invasive fungal disease rather than a specific marker for IA.

Several authors have questioned the specificity of the BDG assay further. Evidence of false positive results due to cellulose haemodialysis membranes [222], intravenous immunoglobulins [223], and antibiotics such as amoxicillin-clavulanic acid [224] has been described. In 2003, Digby et al. found that increased levels of BDG were seen in infected ICU patients both with bacterial and fungal infections compared to noninfected ICU patients [225]. Though the patients in this study were not defined according to EORTC criteria, and insufficient detail on the bacterial and fungal isolates in question was given to properly assess this report, it did suggest that the BDG assay was not specific for fungal infections. Pickering et al. [220] found that 10 of 14 patients with gram positive bacteremia without evidence of invasive fungal disease were BDG positive. However one patient had undergone haemodialysis and other causes of false positives such as the use of cotton gauze could not be ruled out. Based on reactivity of culture supernatants, it has been suggested that patients with Pseudomonas aeruginosa infections may be at risk of producing false positives [226]. In general, these observations of bacteremia resulting in false positives of the BDG test have not been corroborated [217, 227, 228]. Specifically, Racil et al. have examined sera from 26 high risk haematology patients with bacteremia and only 2 were positive for BDG and both of them had invasive fungal infections [229], and Metan et al. [230] found that only 1 of 14 bacteremic patients positive for BDG had no evidence of an invasive fungal infection suggesting that bacteremia is in fact a rare cause of false positives.

6.2. BDG Assays

There are four different commercial assays for the detection of BDG in clinical specimens. The Associates of Cape Cod Fungitell kit uses amoebocyte lysates from Limulus polyphemus while the Seikagaku Fungitec-G test uses reagents from Tachypleus tridentarius as does the Wako β-Glucan test [211]. Recommended cutoffs for reporting positive results vary between assays. Manufacturers of the Fungitell assay requires >80 pg/mL to be detected for a positive with 60–79 pg/mL termed intermediate based the work of Ostrosky-Zeichner et al. [231]. Cutoffs for the T. tridentatus based assays are lower at 20 pg/mL [217] and even lower cutoffs of 11 pg/mL or two sera at 7 pg/mL have been proposed [228]. A fourth assay, GKT-25-M has been reported in the Chinese literature [185].

6.3. Validity of the BDG Assay

A meta-analysis of serum BDG diagnostic accuracy identified 31 studies of invasive fungal infection between 1995 and 2011 for analysis including 17 studies where IA was specifically targeted or identified as a subgroup for analysis [185]. This analysis estimated that the sensitivity for the detection of IFIs was 80% and the specificity was 82%, whilst for IA the figures were 77% and 83%, respectively (Table 2). Significant heterogeneity was found in this analysis. Odabasi et al. [227] examined BDG levels using the Glucatell assay in haematology patients. They proposed a cutoff of 60 pg/mL based on 30 candidemia patients compared to 30 controls, and four patients with Aspergillus pneumonia or fungemia all had BDG levels greater than 60 pg/mL. Ostrosky-Zeichner et al. [231] performed a multicentre study of 163 patients from diverse specialities and invasive fungal disease of whom 22 were diagnosed with proven or probable IA. Based on this dataset, they proposed increasing the cutoff to 80 pg/mL which provided a sensitivity of 64% and specificity of 92.4%. This has been confirmed as a reasonable level by others [230]. Senn et al. [228] looked at neutropenic leukaemia patients and found 15/32 IA cases amongst those with proven or probable fungal disease. Though they did not analyse the IA cases separately, using the Wako -Glucan test and cutoff of 7 pg/mL in two consecutive sera a sensitivity of 63% and specificity of 96% were obtained for invasive fungal disease overall. Using two consecutive sera was backed up by ROC analysis with the area under the ROC curve for 2 sera being 0.87. Comparisons of the BDG and GM test on sera suggest the tests are in most cases comparable for the diagnosis of IA [141, 232, 233], though some studies suggest that BDG may be more likely detected earlier than GM during the development of infection [234]. The BDG assay has generally been applied to haematology patients at risk of IA due to neutrophil deficit, but others have shown the value of this test in intensive care patients [141] and patients with COPD [235]. In an animal model of IA, the BDG assay was applied to BAL as well as serum and was shown in a similar way to GM to both become positive earlier in BAL during the infection course and have a higher sensitivity overall compared to serum [236].

7. Detection of Aspergillus DNA

Soon after the invention of the polymerase chain reaction (PCR) in 1988, reports were being published of how DNA extracts from BAL specimens could be subject to PCR for the detection of Aspergillus DNA and thereby effect a diagnosis in animal models of IA and in patients at risk of IA [237, 238]. Concerns about differentiating between colonisation and infection limited the use of this approach. However, in 1997 Einsele et al. extracted DNA from the blood of neutropenic haematology patients and amplified up part of the large subunit rRNA gene using pan-fungal primers detecting Aspergillus DNA by dot blotting in all of the 13 patients with IA [239]. Since then, there has been extensive interest in this technique. However, due to the fact that, until recently, there were no commercial PCR assays, the main problem has been the publication of multiple assays with differences in DNA extraction, PCR, and product detection with little or no standardisation that prevented easy comparison of study results [240]. A striking visualisation of this diversity can be seen in 29 different protocols in Table 2 of a recent evaluation of PCR protocols [241]. This lack of standardisation leads to the failure to include DNA detection being incorporated into the EORTC-MSG criteria for the definition of invasive fungal infection [242].

7.1. Aspergillus DNA

In Aspergillus sp., DNA, as in all other fungi, is present in both the nucleus and mitochondria and both have been used as targets for diagnostic assays [243]. The genome of A. fumigatus was sequenced in 2005 [244] and has a total size of 29.4 Mbases containing nearly 10,000 genes. Some authors have suggested that unlike GM and BDG, during growth of in vitro Aspergillus, DNA does not appear in the culture supernatant until late in the growth phase when the hyphal cells start to autolyse [245] and this also held true for the more sophisticated human cell-based in vitro model [115] of Hope et al. However, Morton et al. (2010) [111] using a more sensitive PCR assay found that DNA release did occur during exponential growth in vitro.

7.2. PCR Assays

The main advantage of molecular detection is that unlike almost all other detection methods other than culture, there is an element of amplification of the Aspergillus signal and therefore the method has potentially very high sensitivity. Furthermore, PCR methods for the detection of fungal DNA can also be tailored to detect all or most fungi, or members of the genus Aspergillus or a particular Aspergillus sp. through primer and probes design. With many viral infections being diagnosed through PCR-based methods, the technology and expertise is present in most clinical laboratories, and consumables costs for PCR tests, once high, have continued to become more competitive.

Although other biomarkers such as GM and BDG could theoretically be applied to any specimen type, in practice it is only PCR-based methods for DNA detection that have been applied to a wide range of clinical specimens. Respiratory specimens such as BAL and sputum represent obvious material as most cases of IA start as, or compromise wholly of, pulmonary disease. It has been shown that in BALs with high cellularity, positive PCR results are more common, perhaps reflecting the presence of phagocytosed conidia and hyphae in macrophages and neutrophils [94]. Due to the difficulty in obtaining multiple routine specimens, detection of DNA in blood samples has been the focus for much research effort. Furthermore, the presence of Aspergillus DNA in the bloodstream compared to that in respiratory specimens is considered to be less equivocal in terms of clinical significance [246]. Positive results from PCR testing of blood specimens has led to extensive discussion on the nature of the original DNA signal in the specimen. Viable fungus is, unlikely as Aspergillus fungemia, extremely rare [4]. Nonviable Aspergillus cells may be present inside phagocytic cells such as monocytes though many of the patients in question are pancytopenic. It has been shown that platelets bind Aspergillus hyphae and can reduce viability [247], and platelet-bound Aspergillus hyphal fragments may contribute DNA to positive PCR test results. Whether free Aspergillus DNA might circulate in blood is not clear though there have been many successful demonstrations of Aspergillus DNA in serum specimens from patients with IA where centrifugation of the blood suggests that soluble DNA is being detected [248, 249]. In vitro Aspergillus DNA is stable in serum [111], and in animal models it has been determined that Candida DNA can be detected at least 2 hours after inoculation [250]. The uncertainty of which blood fraction to use has led to a variety of fractions being recommended for use in Aspergillus PCR testing including whole blood [241], serum [251], and even blood clots [252]. There is evidence that whole blood is more likely to test positive for Aspergillus DNA than plasma [246, 253]. Most recently a method utilising DNA extracted from both plasma and whole blood provided a very high sensitivity [254]. Other specimens that have been used include CSF [255], tissue, and urine [256, 257].

7.3. DNA Extraction Methods

In order to have effective DNA detection, the Aspergillus DNA within a clinical specimen needs to be purified as much as possible from inhibitory substances and at as high a concentration as possible for amplification. It may also be useful to purify the Aspergillus DNA away from human DNA, as although specific primers and probes will be used for detection, in some PCR assays human DNA in large concentrations can interfere with optimal detection [258]. Broadly, one of the main variations in the method is the initial step where any intact fungal cells are lysed by either enzymic or mechanical means. It has been observed that extraction of DNA from respiratory samples is more straight forward and it has been suggested that a mechanical method such as bead beating is superior for the extraction of Aspergillus DNA from BAL material [259], though good results have also been obtained by others using enzyme-based methods [260] and sensitivities of 80.6% and 88.9% have been calculated from reviews of several studies using this approach [246]. A caveat with enzyme-based methods is that some preparations were identified as a source of contaminating fungal DNA in early studies [261]. Extraction from whole blood is more complex, and many methods propose lysis of red and white blood cells prior to fungal cell lysis and further cleaning up and concentration steps [241, 262]. Attempts to use Aspergillus DNA enrichment techniques to improve sensitivity have proven unsuccessful [263]. Extraction methods may be manual and quite time-consuming or make use of automated extraction machines though usually some manual preextraction steps are required [264]. Recently, the European Aspergillus PCR Initiative (EAPCRI) have, after years of meticulous multicentre evaluation, proposed standards for the extraction of Aspergillus DNA from whole blood [241, 265]. A panel of A. fumigatus spiked blood samples was circulated to 22 centres and by comparing performance with compliance to the protocol standards requested, the EAPCRI laboratory working party was able to determine that factors including use of a large volume of blood (at least 3 mL), bead beating during extraction, and inclusion of an internal PCR control are essential for sensitive and specific assay. This exercise also confirmed the earlier suspicions that, with certain caveats, effective detection of Aspergillus DNA is a function primarily of extraction method and not subsequent amplification. A similar set of proposals for the standardisation of the extraction of Aspergillus DNA from serum has recently been published by the same group [251]. One caveat to these recommendations is that these assays have been developed and validated using blood spiked with Aspergillus conidia though this is not a valid model since although the exact form of the fungus present in blood is not known, it is highly unlikely to be conidial as Aspergillus rarely sporulates in vivo.

7.4. Amplification

All PCRs require a pair of oligonucleotide primers that will bind and prime synthesis of a short stretch of Aspergillus DNA. Of the more widely used nuclear DNA, one of the most popular targets are the genes and spacers of the ribosomal RNA because as in all fungi, in A. fumigatus, and presumably other Aspergillus sp. there are multiple copies though the copy number can vary significantly between strains between 38 and 91 copies [266]. Thus PCRs are to amplify regions of the small subunit (or 18S) rDNA [103, 267–270], large subunit (confusing referred to as 25S, 26S, or 28S) rDNA [248, 271], and intervening transcribed spacers (ITS) 1 and 2 [272, 273]. A multicentre study of PCR assays applied to A. fumigatus DNA extracted from conidia added to whole blood and using 18S and 28S targets suggested that detection of the 28S target was more sensitive and specific though in part this effect was platform specific seen with one particular PCR machine [258]. This was thought to relate in part to the fact that the 18S primers amplified a more conserved sequence and human DNA was coamplified affecting optimal detection of the fungal DNA. Single copy genes such as proteinases [238] and ribotoxin genes [274] have also been used for targets. Mitochondrial DNA targets have been compared with rDNA targets [243] and were shown to have slightly lower analytical sensitivity but slightly superior clinical sensitivity. Despite the wealth of resources of published primers, newly designed primer assays continue to be published [275]. In recent years several groups have described assays combining diagnosis with detection of azole resistance in Aspergillus fumigatus by targeting the CYP51A gene [276–278].

Whilst the polymerase chain reaction in various forms has been the mainstay of molecular detection technology, nucleic acid sequence-based amplification (NASBA) methods to detect Aspergillus RNA have been described [279]. NASBA is considered by some to be more robust than PCR with the advantages of requiring less specimen, using isothermal amplification and is less likely to have contamination problems from fungal DNA in enzymes used for extraction [280]. Real time NASBA methods have been developed [281, 282], and in an animal model compared to PCR [283] NASBA appears to be sensitive. When applied to clinical specimens from patients with IA, detection of total nucleic acids by NASBA has also shown good sensitivity [284]. Morton et al. have investigated reverse transcriptase methods to detect rRNA in blood in a murine model of IA and found this approach to have potential where effective systems for stabilisation and isolation of RNA are used [285].

7.5. PCR Product Detection

Real-time (RT) PCR products can be detected either by a generic stain such as SYBR green or more commonly using a specific probe, first described by Loeffler et al. in 2000 [286], and this has become a standard, involving the use of hydrolysis [287, 288] and hybridisation probes [249]. RT PCR has advantages of speed, reduced contamination as no post-PCR manipulation is required, increased sensitivity and specificity, the potential to reduce costs through low volume and low reagent costs, and quantification of signal. However, Johnson et al. [257] have argued that there has a been a lack of detail in published studies on RT PCR methods for the detection of Aspergillus DNA, needed to understand the wide range of analytical and clinical sensitivities reported. They advocate the use minimum information for the publication of real-time quantitative PCR experiments (MIQE) and report a RT PCR assay fulfilling these guidelines and demonstrating good performance in vitro and on clinical specimens from patients with proven or suspected IA [257]. In an effort to improve both sensitivity and specificity, several authors have described nested-PCR assays where an initial product is subject to a second round reaction with new primers [289, 290]. However, most authorities regard this approach as flawed as it requires post-PCR manipulations and increases the risk of contamination and false positives, though studies using nested-PCR methods continue to be published [255, 291]. Many PCR assays only target A. fumigatus, the most common species. In order to ensure that all species of Aspergillus are detected, one approach is to amplify a region of DNA conserved in Aspergillus spp. and to use probes specific for each species [103, 292]; alternatively, products can often be identified using a single probe and melting curve analysis [257, 270]. These approaches are likely to be useful in centres where a significant proportion of cases are caused by non-fumigatus spp. ELISA systems for the detection of PCR products have also been developed for Aspergillus DNA detection, and though effective, they have been found to be less easy to work with than RT-PCR methods [293]. It may seem remarkable that as recently as 2009 block-based PCR assays with detection by running out products by gel electrophoresis and staining with ethidium bromide have been published [269], though White and Barnes have reported that sensitivities of conventional and real-time PCRs are equivalent whilst the specificity of conventional PCR tends to be lower [246].

In recent years, commercial PCR kits have been launched providing standardisation and a high level of quality control in the development and manufacture of the kits. The Roche Diagnostics Septifast is designed to detect a range of microbial pathogens from blood including A. fumigatus. In studies of haematology patients, A. fumigatus has been detected in blood samples though the diagnostic comparator in these studies was blood culture which was unsurprisingly negative [294, 295]. In a study of three patients with probable IA as defined by EORTC-MSG criteria, all were positive by Septifast for Aspergillus DNA. The test was also positive for one patient with no evidence of IA [296]. Case reports of this assay being of use in the diagnosis of IA in liver transplant recipients [297] and a case of Aspergillus endocarditis have been described [298]. Myconostica have recently launched the Mycassay Aspergillus PCR kit which has been compared with a well-established in-house assay and compared favourably in terms of sensitivity in serum [299], BAL specimens [300], and also lung tissue [301].

As in the case of other serological assays, improving the specificity of PCR tests for Aspergillus DNA by requiring two consecutive positive results has been considered [246]. This approach has been shown convincingly to enhance specificity without compromising sensitivity in studies where patients with febrile neutropenia were serially screened [275, 302].

7.6. Validity of PCR

A meta-analysis of PCR methods applied to whole blood, serum and plasma to detect IA was published in 2009 [183], examining 16 studies published between 2000 and 2008. Analysis using a single positive PCR gave an overall sensitivity of 88% and specificity of 75% whilst requiring two positive samples reversed the figures with 75% sensitivity and 87% specificity (Table 2). The majority of studies involved adults with haematological malignancies or undergoing stem cell transplantation; however, some studies also looked at patients undergoing solid organ transplantation and two dealt with paediatric patients. There were too few studies to carry out subgroup analysis though. Studies published since then have typically demonstrated the continued variation in reported performance with some studies on achieving sensitivities as low as 50% [243] and others 100% [254], with most studies in between [275, 293, 303]. Some studies in paediatric patients have demonstrated a complete lack of sensitivity of PCR [304] whilst in others sensitivities are similar to those seen in adult patients [291, 305]. This continued variation probably reflects the delays in the ability to adopt proposed standardised methods together with the realisation of the effects of concomitant antifungal therapy in patients who are tested (see below). Sun et al. [306] have published a meta-analysis of the use of BAL material for the PCR diagnosis of IA. They reviewed 17 studies that fitted the inclusion criteria between 1993 and 2009, including several pre-EORTC criteria studies where the criteria used for the definition of IA were deemed similar. Most studies focussed on patients with haematological malignancy and stem cell transplantation though a number of patients with solid tumours were also included. Overall sensitivity was high at 91% in proven and probable IA, with specificity 92% and a diagnostic odds ratio of 122. The authors commented on the variations in methodology and noted that commercial extraction systems appear to improve specificity though not sensitivity. Avni et al. [10] more recently have also published a meta-analysis including several more recent studies though this has not changed the sensitivity, and the overall specificity was slightly increased at 96%. These authors reviewed 10 studies where GM and PCR were directly compared on BAL samples. In seven studies where GM with a cutofff of 0.5 was compared to PCR, sensitivities and specificities (GM 82%, 97%; PCR 86% and 97%, resp.) were comparable. The results suggest combining both methods to maximise performance as has been advocated by others [89, 293, 307], an approach largely limited by cost. The GM assay unlike PCR is part of the EORTC criteria for defining probable cases of IA [308], and at-risk patients with relevant positive CT signs but negative GM (and other mycological results) are classified as possible IA. Bergeron et al. [38] have found that 66% of patients with possible IA in a recent study were PCR positive suggesting that if PCR-based assays can be standardised the assay can be incorporated into the EORTC criteria and many possible patients could be upgraded to probable disease leading to improved outcomes.

The effect of antifungal therapy on the sensitivity of PCR assays for IA has long been debated and McCulloch et al. 2012 suggest that their animal model shows evidence that antifungal therapy in an animal model reduces the rate of PCR detection [309]. Reinwald et al. 2012 systematically examined the effect of prior mould active antifungal therapy on the sensitivity of PCR on BALS specimens and demonstrated a decreased sensitivity where patients had received more than one agent prior to bronchoscopy [310]. This supports the findings from the AmBiLoad (high doses liposomal amphotericin B) trial where Hummel et al. 2010 attributed the low sensitivities of PCR testing to the use of AmBisome/AmBiLoad [311], and others have made similar observations in paediatric patients [312]. This contrasts with the findings of Musher et al. who found improved sensitivity for PCR detection of AI in BAL samples in patients on antifungal therapy compared to those who had not [313]. As these authors point out, this kind of analysis is problematic due to being subject to significant bias in terms of who is selected for antifungal therapy. In animal models where this bias can be overcome, treatment of IA reduces the sensitivity of all diagnostic tests reflecting the overall reduction of the burden of the fungus [103].

8. Other Biomarkers for IA

A recent test that has been developed and marketed for the detection of Aspergillus and diagnosis of IA is an antigen test detecting an extracellular glycoprotein antigen only produced during active growth of the fungus using a lateral flow device format [314]. The assay is specific for Aspergillus sp. and reacted positively to sera from patients diagnosed with IA by GM and BDG assay results [314, 315]. In a guinea pig model of IA, the assay flagged earlier than either GM or BDG [316]. Other A. fumigatus antigens that have been suggested as targets for a new assay include Cf2 on the surface of the growing fungus [317], other cell-wall associated antigens [318], proteinases [319] the proteins of the immunosecretome [320], and gliotoxin and its derivatives [321, 322].

Serum antibodies to Aspergillus have been suggested as a diagnostic approach for detection of IA; however, in the immunocompromised patient populations affected by this infection, antibody responses generally are poor [119]. Antibody assays may be useful in the case of IA seen in nonneutropenic patients [323, 324], or in the case of identifying patients at risk of IA prior to myeloablative chemotherapy, or stem cell transplantation [325]. Antibody responses to Aspergillus in patients with IA in a nonimmunocompromised background such as COPD have been discounted [48] but may in fact have a useful role (Datta et al., manuscript submitted).

Breath tests for pulmonary IA have been proposed for many years and a recent report of the successful detection of the 2-pentyl-furan in the breath of 2 patients with IA that resolved on treatment suggests that this novel approach may have provided evidence of proof of concept [326] and trials of this ultra-low interventional investigation are eagerly awaited.

9. Strategies

Given an increasing number of diagnostic tools, many of which have been shown to perform well, the clinician managing a patient population at risk of IA needs to determine a strategy for when to intervene to provide best outcomes. A range of approaches to this problem have been formulated, whilst various terms using these approaches can be broadly categorised as prophylaxis, empiric, preemptive, and targeted (Table 4) [327].

Table 4: Approaches to the prevention and diagnosis of IA.

Strategy
Rationale
Laboratory diagnostic use

Prophylaxis
Prevention of infection using antifungal treatment and protective accommodation
None

Empiric
Early antifungal therapy in response to non-specific signs and symptoms
None (blood cultures are typically done to detect bacteremia and fungemia)

Preemptive
Antifungal therapy in response to early specific markers of IA
CT, GM, PCR, and BDG usually one or two markers triggering therapy

Targetted
Antifungal therapy of clearly defined cases of IA
All available investigations, using EORTC-MSG criteria

Use of antifungal therapy with or without protective HEPA-filtered accommodation to prevent susceptible patients from succumbing to IA has been intensively researched and is controversial [328, 329]; however, most institutions will treat patients at risk of IA prophylactically. Effective prophylaxis will reduce reliance of laboratory diagnosis significantly and where this reduces pretest probabilities of IA in patient populations, the effectiveness of expensive laboratory tests is likely not to be cost-effective [330]. The emergence of resistance to azole antifungals, the mainstay of prophylaxis in A. fumigatus, in recent years [331], though not currently thought to result from prophylaxis, has led many to question the use of this approach. Empiric antifungal therapy has been the main approach in many centres for patients with haematological malignancies and undergoing stem cell transplantation, typically where patients are febrile and fail to respond to antibacterial therapy [332]. Laboratory investigations are either not carried out, or, if done, results are looked for to confirm the strategy and are possibly used to escalate or de-escalate the therapy. This strategy typically using amphotericin B is considered to improve survival [333], though there are very few trials against placebo and these only showed improvements in mortality attributed to invasive fungal infection and not overall mortality [334]. However, it has been estimated that 40%–50% of all neutropenic patients receive empiric antifungal therapy whilst only 5%–15% have infections [327]. Thus this is not an efficient approach, exposing many patients to unnecessary medication with concomitant risk [335] and the cost-effectiveness has been questioned [336]. It has also been suggested that fever is not only nonspecific but also may be a late marker for invasive fungal disease [337].

Thus some form of preemptive strategy utilising one or more specific markers for IA have been advocated by many for several years [335]. Retrospective studies of using HRCT to guide antifungal therapy in patients at risk from IA has shown to lead to earlier therapy [338, 339]. Serial CT scanning has been found in some studies to show signs of IA prior to serum GM [340]; however, for many centres there are likely to be logistic limitations to obtaining regular serial CT scans. Several strategies for the incorporation of rapid nonculture-based tests such as GM, BDG, and PCR together with HRCT investigations into management strategies have been proposed, stratified by current prophylaxis and risk of infection [337]. Individual studies of the effectiveness of these strategies include Maertens et al. [341] analysis of the use of daily GM screening combined with HRCT and bronchoscopy in neutropenic patients resulting in reduced antifungal use and earlier therapy in several patients. The importance of incorporating any strategy into a clinical or integrated care pathway which is systematic, multidisciplinary, and auditable has been argued [342]. Barnes et al. [343] incorporated GM and PCR into a neutropenic care pathway identifying 17 cases of probable or possible IA, reducing antifungals costs and with no excess mortality compared to previous years. Cuenca-Estrella looked at how to combine PCR and GM suggesting using two positive PCR test results together with GM for optimal performance [275]. They noted that positive PCR tests most often preceded GM positivity and HRCT signs. Girmenia et al. [344] described a pathway with the use of GM/CT-based investigations prompted by persistent febrile neutropenia finding 63% survival in patients with IA and reduced antifungal use. Millon et al. looked at applying PCR to GM positive specimens but found that this was often not useful in aiding the distinction between true and false GM positives but that overall combining PCR and GM testing to inform treatment decisions was the way forward [345].

The European Conference on Infections in Leukaemia (ECIL) published a review of biomarker use recommending diagnostic-driven strategy in haematological oncology patients with GM testing every 3-4 days together with clinical evaluations and HRCT [346]. While this publication accepted that there is moderate evidence for the use of BDG assay again in conjunction with other investigations, they stopped short of a recommendation of its incorporation into a routine diagnostic strategy citing issues that need resolving including the understanding of the value BDG screening compared to preemptive assays, the value of the assay in HRCT recipients and paediatric patients and in specimens other than sera, the integration of the assay with other markers, and the outcomes in patients where BDG is used in a diagnostic strategy. Perhaps surprisingly, the ECIL recommendations failed to endorse the use of PCR testing in haematological malignancy due to a lack of standardization [295]. A set of German guidelines on managing IA accepted that both empiric and preemptive strategies could be effective [347]. At a recent consensus conference on invasive fungal infections in 2010, it was suggested that while a diagnostic-driven strategy is what should be aimed for, the role of at least some screening assays in a diagnostic-driven approach may be unsuitable in patients on mould-active antifungal prophylaxis [348].

Targetted approaches to managing IA and other IFD either requiring evidence of proven disease through positive culture from a sterile site or histopathological evidence of tissue invasion, or probable disease defined by two or more positive signs or markers is in practice rarely used due to the risks of delay in starting therapy and the associated poorer response to therapy.

The gold standard of analysis in clinical research is the random controlled trial (RCT) and there are no theoretical reasons why different diagnostic strategies cannot be subject to the same rigorous comparisons [349] except for the high cost and logistic difficulty. However, some RCTs of diagnostic approaches for IA or invasive fungal infections in at-risk patients have been reported. In an attempt to utilise the potential of the enhanced sensitivity and high positive predictive value of testing of PCR, Hebart et al. [350] randomised a cohort of allogeneic stem cell transplant patients to receive one-arm antifungal therapy after a single positive pan-fungal PCR or had febrile neutropenia unresponsive to antibacterial therapy or had in the other arm simple empiric therapy. The group with PCR-directed therapy received more antifungal therapy and showed better survival after 30 days (1.5% versus 6.3%) but not after 100 days. Eight cases of proven IA were seen in the PCR group and 5 in the control in both groups. Overall, the findings were perhaps disappointing but the results did suggest that a higher frequency of PCR screening might detect invasive fungal infections earlier than an empiric approach.

In a similar study of reduced intensity, conditioning allogenic stem cell transplantation patients were screened with an Aspergillus specific PCR test and patients with a single positive result were randomised for antifungal therapy with liposomal amphotericin or no intervention though all febrile neutropenic patients received antifungals on an empiric basis [351]. Interestingly in this study a single positive PCR result was found not to be associated with invasive fungal infection within the first 100 days after transplant; however, the value of PCR was in part not possible to determine due to the low number of cases of infection during this period. Furthermore, over half the patients with a single positive PCR result were not randomised due to clinicians rebelling against the use of intravenous antifungals in otherwise well patients. In all 20 of the cases of these patients with a single positive PCR result, the test failed to be reproducible. An alternative study design was adopted by Cordonnier et al. [352] who randomised a group of patients with haematological malignancies or autologous stem cell transplant recipients to receive either standard empiric antifungal therapy in the case of antibiotic resistant febrile neutropenia or to a preemptive therapy protocol. In the preemptive group, empiric therapy was withheld unless there was clinical or imaging evidence of fungal infection or a positive GM result, though a higher cutoff of 1.5 was being used at this time. There was no difference in survival between the groups though there were significantly more invasive fungal infections in the preemptive group (9.1% compared to 2.7%), and most of these were IA. Antifungal costs in the preemptive group were reduced by 35%. This study had several limitations such as the relatively high GM cutoff used, the low frequency use of this assay, and the omission of some high-risk patients [335]. However, this study has encouraged others to plan further RCTs with the adoption of diagnostic tests with high negative predictive values or logistic ratios in order to rule out fungal infections including IA where results are negative in patients being screened [353]. A mixed treatment analysis of empiric therapy compared to two of the above preemptive therapy approaches found no difference in all-cause mortality [354].

10. Using Laboratory Tests to Predict Outcomes

Efforts to improve the performance of diagnostic tests frequently focus on comparative studies and devising increasingly detailed “gold standard” case definitions. However, this leads to tests simply defining patients who fit into arbitrary diagnostic criteria and there has been a move in more recent years to understand the relationship between diagnostic tests for IA with clinical outcomes enabling clinicians not just to diagnose but also to predict outcomes to antifungal therapy and use the tests to monitor response. This linking of diagnostic test results to the outcome of therapy may also allow the tests to stand as surrogate markers in antifungal drug trials [355]. Simple correlations of the dynamics of serum GM and positive patients becoming negative with clinical outcome survival indicate a good correlation in individual studies [356–358] confirmed in a recent literature review [359]. In a more sophisticated analysis, Koo et al. [360] looked quantitatively at serum GM dynamics earlier in the disease process with outcomes in patients on antifungal therapy. They found a correlation between baseline GM levels and survival at 6 weeks. They were also able to quantify what many had observed anecdotally or in earlier studies [361, 362] that in patients with proven or probably IA for each unit rise in GM index with a 7-day period following diagnosis increased the risk of 6-week mortality by 25% and a decline of 1 unit reduced this risk by 22%. A similar exercise to this examining GM trajectories in patients compared to general clinical response and 12-week mortality also showed a correlation between GM decline and outcome in terms of clinical response, though not in terms of survival in patients with a positive (≥0.5) baseline GM result. However, in patients with a negative (<0.5) baseline GM, there was a clear correlation between increasing GM levels and both clinical response and survival at week 12 [363]. The authors used ROC analysis to demonstrate that any patient showing with a baseline GM of <0.5 and showing an increase of >0.13 within 2 weeks of baseline measurements increased the likelihood of mortality by week 12 by 2.4-fold. Bergeron et al. [358] did not find a correlation of changes in GM level in the first 10 days after a positive sample with outcome, but did see an overall correlation between baseline GM levels and 9-week survival.

Nouer et al. have proposed incorporating GM dynamics into a new set of response criteria in patients diagnosed by a positive GM, where success is defined by the GM assay is becoming negative and remains negative for two or more weeks and failure by the persistent presence of GM in serum [11] GM does appear to be more a highly responsive marker for IA and was shown to decline to negative levels in 87% of patients who responded according to these criteria within 3 weeks. Combining analysis of GM normalisation with baseline neutrophil levels and creatine clearance may enhance the prediction of outcomes in IA and provide a simple way to optimise management. In the earliest studies of molecular diagnosis of IA, persistent positive PCR results were more likely to be seen in patients who did not survive, whilst patients whose blood became negative had better outcomes [239]. Furthermore, this same group [364] showed that in prior to undergoing bone marrow transplantation, patients with BAL specimens positive by PCR for Aspergillus were predictive of those developing IA during transplantation. Bergeron et al. [358] did not find any difference in outcomes in patients testing positive by a PCR assay for Aspergillus compared to those who did not. But in IA patients serially tested for Aspergillus RNA by NASBA, those dying whose death was attributed to IA were more likely to have became positive or remained positive for the NASBA test [365]. An analysis of changes in BDG levels in patients with a range of IFIs including IA found that short-term BDG increases did not correlate with survival and that BDG does decline but over a longer term which is of less practical clinical use [366]. Examination of the dynamics of general markers of inflammation such as C-reactive protein and interleukin 6 showed that a failure of these markers to decline after initiation of antifungal therapy was predictive of a poor response [65].

11. Conclusions

A vast effort has been expended and continues to be expended on the aim of being able to identify patients who have IA and who will benefit from some form of therapy. This reflects the continued disproportionate mortality associated with this disease despite major improvements in antifungal therapy together with a desire to manage patients at risk of IA more efficiently and with lower costs by targeting therapies [330].

Immunocompromised patient populations at risk, particularly those with low neutrophil counts, namely, those with haematological malignancies and undergoing stem cell transplantation, have been recognised for decades whilst there is also considerable understanding in other groups such as those with solid organ transplantation. Increasingly there is interest in risk of IA and methods of diagnosis in immunocompetent patient groups such as those with chronic lung disease which may require a very different approach [367].

Of the wide variety of methods reviewed of diagnosing IA, direct microscopy and histopathology are undoubtedly the most subjective, skilled, and labour intensive. Though histopathological detection of Aspergillus of tissue will remain an essential capacity and help define the highest level of certainty in diagnostic criteria [368], less invasive and more rapid methods have already overtaken this approach in most settings. Some will also consider that traditional culture-based methods may also be superceded by DNA and antigen detection methods. However, in the recent US PATH registry update culture of Aspergillus for the diagnosis of IA was still the most frequent laboratory approach [369]. Furthermore, cultures of Aspergillus allow further analysis such as susceptibility to testing, recent developments in direct molecular detection of resistance notwithstanding, and the possibility of molecular typing in epidemiological investigations [370]. Furthermore, new species of Aspergillus causing invasive disease continue to be uncovered by culture whose applicability to serological and molecular detection cannot be assumed [27]. Culture of respiratory specimens in clinical laboratories is unlikely to be abandoned in the near future and culture of Aspergillus will remain an important if generally insensitive approach to the diagnosis of IA.

Chest HRCT scanning for the presumptive diagnosis of pulmonary IA has revolutionised approaches to this disease in recent decades and become the third pillar of the probable category of IA. However, CT signs still lack specificity and it remains to be seen if developments in methods to provide a more specific identification of lesions as relating to Aspergillus will lead to a second revolution and the reduction in need to send specimens to the pathology laboratory.

The detection of galactomannan in clinical specimens is firmly established as the test of choice for any laboratory providing diagnostic services for patients at risk of IA. Serum detection remains a key approach and amenable to serial measurements whilst BAL material appears to have a higher sensitivity but is often harder to obtain. False positives are less of an issue than is often claimed with antibiotic sources of GM now rarely seen and neonatal samples likely to account for a tiny fraction of samples analysed. Sensitivity is clearly affected by antifungal treatment, though the biological basis for this is unclear, this remains the main limitation to the use of the assay particularly in patients undergoing antifungal prophylaxis. A plethora of meta-analyses have confirmed the clinical value of GM testing and at least some analyses of GM serum kinetics point to the potential for this assay to guide therapy beyond diagnosis. The BDG assay has yet to be widely adopted as a diagnostic tool, perhaps suffering from the need to also require more specific diagnostic methods to target therapy in positive patients. Meta-analysis suggests that problems with specificity were probably overestimated in initial studies and sensitivity is comparable with GM. The BDG assay will probably find its place in some centres in carefully designed care pathways where the negative predictive value can be used to reduce empiric therapy. The PCR assay to detect Aspergillus DNA held a large amount of promise but has been limited up until recently by a lack of standardisation. The scientists of EAPCRI have nobly met the challenge of technical diversity in PCR assays and provided meticulously researched standard methods for extraction of DNA from whole blood and serum. The continuing introduction of commercial PCR assays will consolidate this standardisation. These advances are likely to lead to easier comparisons with other methods and incorporation of this form of test into the EORTC criteria for research use. Preemptive therapy is based on assessing risk in patients as fully as possible, and increasingly underlying aspects of disease and routine cell and biochemical markers are being found to be relevent to this assessment. In a recent fascinating examination of patients with IA it was shown that patients with allogeneic SCT were more likely to exhibit airways rather than angio-invasive disease (as shown by HRCT) and higher leukocyte counts and were more likely to provide a positive culture yield on bronchoscopy compared to patients with acute leukaemia [38]. How to decide on the best blood-based assay to use and in what way has exercised the minds of haematologists and clinical microbiologists for some time. This is an area where opinions are divided. It is difficult to reconcile statements such as “highly sensitive and specific methods for the detection of an early fungal infection are yet unavailable” made in 2012 [371] with significant successes of others using a preemptive approaches using antigen and PCR detection [343]. It is generally agreed that an RCT of empiric compared to preemptive diagnostic-driven therapy, probably comparing two or more laboratory tests [353], is the way forward, though the few undertaken so far have had significant limitations. Ensuring rapid diagnosis as delays may impact on long-term outcomes [61]. To the authors knowledge, currently two more such studies are underway an Australian study which was started in 2005 but has still to report (NCT00163722) an EORTC sponsored study started in 2012 (NCT01288378). Others have made the case to compare preemptive approach with a patient population treated with antifungal prophylaxis [335].

New assays continue to be described and many will doubtlessly fall at early hurdles due to poor performance or lack of investment whilst competing against many suboptimal but well-established competitors. Predicting the future of developments in the diagnosis of IA is probably harder than predicting outcomes in the disease itself, but this author is particularly interested to see positive developments in the minimally invasive breath tests and RNA detection with its promise of detecting actively growing as compared to colonising Aspergillus.

People with fewer than the normal level of neutrophils continue to die of IA despite all the developments in diagnosis and treatment. It a cliché but also the truth to say that the challenge continues and the improvements in outcomes seen in the last decades can be built upon as we continue to understand the complex interaction between the fungi of the genus Aspergillus and humans with damaged host defences.

References

J. P. Latge, “Aspergillus fumigatus and aspergillosis,” Clinical Microbiology Reviews, vol. 12, pp. 310–350, 1999.

W. W. Hope, T. J. Walsh, and D. W. Denning, “The invasive and saprophytic syndromes due to Aspergillus spp.,” Medical Mycology, vol. 43, supplement 1, pp. S207–S238, 2005.

Z. Erjavec, H. Kluin-Nelemans, and P. E. Verweij, “Trends in invasive fungal infections, with emphasis on invasive aspergillosis,” Clinical Microbiology and Infection, vol. 15, no. 7, pp. 625–633, 2009.

R. Duthie and D. W. Denning, “Aspergillus fungemia: report of two cases and review,” Clinical Infectious Diseases, vol. 20, no. 3, pp. 598–605, 1995.

J. J. Tarrand, M. Lichterfeld, I. Warraich et al., “Diagnosis of invasive septate mold infections: a correlation of microbiological culture and histologic or cytologic examination,” American Journal of Clinical Pathology, vol. 119, no. 6, pp. 854–858, 2003.

C. R. Thornton, “Detection of invasive aspergillosis,” Advances in Applied Microbiology, vol. 70, pp. 187–216, 2010.

S. Ascioglu, B. E. de Pauw, J. P. Donnelly, and L. Collette, “Reliability of clinical research on invasive fungal infections: a systematic review of the literature,” Medical Mycology, vol. 39, no. 1, pp. 35–40, 2001.

S. Ascioglu, J. H. Rex, B. de Pauw et al., “Defining opportunistic invasive fungal infections in immunocompromised patients with cancer and hematopoietic stem cell transplants: an international consensus,” Clinical Infectious Diseases, vol. 34, no. 1, pp. 7–14, 2002.

B. De Puaw, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

T. Avni, I. Levy, H. Sprecher, et al., “Diagnostic accuracy of PCR alone and compared to galactomannan in bronchoalveolar lavage for the diagnosis of invasive pulmonary aspergillosis: systematic review,” Journal of Clinical Microbiology, vol. 50, no. 11, pp. 3652–3658, 2012.

S. A. Nouer, M. Nucci, N. S. Kumar, et al., “Earlier response assessment in invasive aspergillosis based on the kinetics of serum Aspergillus galactomannan: proposal for a new definition,” Clinical Infectious Diseases, vol. 53, pp. 671–676, 2011.

F. Traunmuller, M. Popovic, K. H. Konz, et al., “Efficacy and safety of current drug therapies for invasive aspergillosis,” Pharmacology, vol. 88, pp. 213–224, 2011.

D. Neofytos, J. A. Fishman, D. Horn et al., “Epidemiology and outcome of invasive fungal infections in solid organ transplant recipients,” Transplant Infectious Disease, vol. 12, no. 3, pp. 220–229, 2010.

D. Neofytos, D. Horn, E. Anaissie et al., “Epidemiology and outcome of invasive fungal infection in adult hematopoietic stem cell transplant recipients: analysis of multicenter Prospective Antifungal Therapy (PATH) alliance registry,” Clinical Infectious Diseases, vol. 48, no. 5, pp. 265–273, 2009.

T. J. Walsh, R. W. Finberg, C. Arndt, et al., “Liposomal amphotericin B for empirical therapy in patients with persistent fever and neutropenia. National Institute of Allergy and Infectious Diseases Mycoses Study Group,” The New England Journal of Medicine, vol. 340, pp. 764–771, 1999.

N. Wu, Y. Huang, Q. Li, C. Bai, H. D. Huang, and X. P. Yao, “Isolated invasive Aspergillus tracheobronchitis: a clinical study of 19 cases,” Clinical Microbiology and Infection, vol. 16, no. 6, pp. 689–695, 2010.

E. Kazan, J. Maertens, R. Herbrecht et al., “A retrospective series of gut aspergillosis in haematology patients,” Clinical Microbiology and Infection, vol. 17, no. 4, pp. 588–594, 2011.

S. R. Mays, M. A. Bogle, and G. P. Bodey, “Cutaneous fungal infections in the oncology patient: recognition and management,” American Journal of Clinical Dermatology, vol. 7, no. 1, pp. 31–43, 2006.

C. Y. Chen, W. H. Sheng, A. Cheng, et al., “Invasive fungal sinusitis in patients with hematological malignancy: 15 years experience in a single university hospital in Taiwan,” BMC Infectious Diseases, vol. 11, article 250, 2011.

P. Parize, M. O. Chandesris, F. Lanternier et al., “Antifungal therapy of aspergillus invasive otitis externa: efficacy of voriconazole and review,” Antimicrobial Agents and Chemotherapy, vol. 53, no. 3, pp. 1048–1053, 2009.

J. I. Pitt, “The current role of Aspergillus and Penicillium in human and animal health,” Journal of Medical and Veterinary Mycology, Supplement, vol. 32, supplement 1, pp. 17–32, 1994.

W. J. Steinbach, K. A. Marr, E. J. Anaissie, et al., “Clinical epidemiology of 960 patients with invasive aspergillosis from the PATH Alliance registry,” Journal of Infection, vol. 65, no. 5, pp. 453–464, 2012.

C. Lass-Flörl, K. Griff, A. Mayr et al., “Epidemiology and outcome of infections due to Aspergillus terreus: 10-Year single centre experience,” British Journal of Haematology, vol. 131, no. 2, pp. 201–207, 2005.

E. Mokaddas, M. H. A. Burhamah, S. Ahmad, and Z. U. Khan, “Invasive pulmonary aspergillosis due to Aspergillus terreus: value of DNA, galactomannan and (1→3)-β-D-glucan detection in serum samples as an adjunct to diagnosis,” Journal of Medical Microbiology, vol. 59, no. 12, pp. 1519–1523, 2010.

S. Krishnan, E. K. Manavathu, and P. H. Chandrasekar, “Aspergillus flavus: an emerging non-fumigatus Aspergillus species of significance,” Mycoses, vol. 52, no. 3, pp. 206–222, 2009.

A. Chakrabarti, S. S. Chatterjee, A. Das, and M. R. Shivaprakash, “Invasive aspergillosis in developing countries,” Medical Mycology, vol. 49, supplement 1, pp. S35–S47, 2011.

J. A. Sugui, S. W. Peterson, L. P. Clark, et al., “Aspergillus tanneri sp. nov., a new pathogen that causes invasive disease refractory to antifungal therapy,” Journal of Clinical Microbiology, vol. 50, pp. 3309–3317, 2012.

S. A. Balajee, J. L. Gribskov, E. Hanley, D. Nickle, and K. A. Marr, “Aspergillus lentulus sp. nov., a new sibling species of A. fumigatus,” Eukaryotic Cell, vol. 4, no. 3, pp. 625–632, 2005.

T. Yaguchi, Y. Horie, R. Tanaka, T. Matsuzawa, J. Ito, and K. Nishimura, “Molecular phylogenetics of multiple genes on Aspergillus section Fumigati isolated from clinical specimens in Japan,” Nihon Ishinkin Gakkai Zasshi, vol. 48, no. 1, pp. 37–46, 2007.

S. J. Howard, E. Harrison, P. Bowyer, et al., “Cryptic species and azole resistance in the Aspergillus niger complex,” Antimicrobial Agents and Chemotherapy, vol. 55, pp. 4802–4809, 2011.

L. Alcazar-Fuoli, E. Mellado, A. Alastruey-Izquierdo, M. Cuenca-Estrella, and J. L. Rodriguez-Tudela, “Aspergillus section Fumigati: antifungal susceptibility patterns and sequence-based identification,” Antimicrobial Agents and Chemotherapy, vol. 52, no. 4, pp. 1244–1251, 2008.

R. D. Meyer, L. S. Young, D. Armstrong, and B. Yu, “Aspergillosis complicating neoplastic disease,” The American Journal of Medicine, vol. 54, no. 1, pp. 6–15, 1973.

R. D. Diamond, R. Krzesicki, B. Epstein, and W. Jao, “Damage to hyphal forms of fungi by human leukocytes in vitro. A possible host defense mechanism in aspergillosis and mucormycosis,” American Journal of Pathology, vol. 91, no. 2, pp. 313–328, 1978.

T. F. Patterson, “Risks stratification for invasive aspergillosis: early assesment of host susceptibility,” Medical Mycology, vol. 47, supplement 1, pp. S255–S260, 2009.

L. Li, J. Wang, W. Zhang, et al., “Risk factors for invasive mold infections following allogeneic hematopoietic stem cell transplantation: a single center study of 190 recipients,” Scandinavian Journal of Infectious Diseases, vol. 44, pp. 100–107, 2012.

M. C. Nicolle, T. Benet, A. Thiebaut, et al., “Invasive aspergillosis in patients with hematologic malignancies: incidence and description of 127 cases enrolled in a single institution prospective survey from 2004 to 2009,” Haematologica, vol. 96, pp. 1685–1691, 2011.

O. Lortholary, J. P. Gangneux, K. Sitbon, et al., “Epidemiological trends in invasive aspergillosis in France: the SAIF network (2005–2007),” Clinical Microbiology and Infection, vol. 17, pp. 1882–1889, 2011.

A. Bergeron, R. Porcher, A. Sulahian, et al., “The strategy for the diagnosis of invasive pulmonary aspergillosis should depend on both the underlying condition and the leukocyte count of patients with hematologic malignancies,” Blood, vol. 119, pp. 1831–1837, 2012.

M. T. Montagna, G. O. De, C. Napoli, et al., “Invasive fungal infections in patients with hematologic malignancies (aurora project): lights and shadows during 18-months surveillance,” International Journal of Molecular Sciences, vol. 13, pp. 774–787, 2012.

L. Slobbe, S. Polinder, J. K. Doorduijn et al., “Outcome and medical costs of patients with invasive aspergillosis and acute myelogenous leukemia-myelodysplastic syndrome treated with intensive chemotherapy: an observational study,” Clinical Infectious Diseases, vol. 47, no. 12, pp. 1507–1512, 2008.

M. Rosenhagen, R. Feldhues, J. Schmidt, T. Hoppe-Tichy, and H. K. Geiss, “A risk profile for invasive aspergillosis in liver transplant recipients,” Infection, vol. 37, no. 4, pp. 313–319, 2009.

S. M. Hosseini-Moghaddam and S. Husain, “Fungi and molds following lung transplantation,” Seminars in Respiratory and Critical Care Medicine, vol. 31, no. 2, pp. 222–233, 2010.

M. Pacholczyk, B. Lagiewska, W. Lisik, et al., “Invasive fungal infections following liver transplantation—risk factors, incidence and outcome,” Annals of Transplantation, vol. 16, pp. 14–16, 2011.

M. K. Ju, D. J. Joo, S. J. Kim et al., “Invasive pulmonary aspergillosis after solid organ transplantation: diagnosis and treatment based on 28 years of transplantation experience,” Transplantation Proceedings, vol. 41, no. 1, pp. 375–378, 2009.

R. E. Lewis and D. P. Kontoyiannis, “Invasive aspergillosis in glucocorticoid-treated patients,” Medical Mycology, vol. 47, supplement 1, pp. S271–S281, 2009.

A. Russo, M. Falcone, A. Vena, et al., “Invasive pulmonary aspergillosis in non-neutropenic patients: analysis of a 14-month prospective clinical experience,” Journal of Chemotherapy, vol. 23, pp. 290–294, 2011.

J. Garbino, U. Fluckiger, L. Elzi, et al., “Survey of aspergillosis in non-neutropenic patients in Swiss teaching hospitals,” Clinical Microbiology and Infection, vol. 17, pp. 1366–1371, 2011.

F. Ader, “Invasive pulmonary Aspergillosis in patients with chronic obstructive pulmonary disease: an emerging fungal disease,” Current Infectious Disease Reports, vol. 12, no. 6, pp. 409–416, 2010.

M. Falcone, A. P. Massetti, A. Russo, V. Vullo, and M. Venditti, “Invasive aspergillosis in patients with liver disease,” Medical Mycology, vol. 49, no. 4, pp. 406–413, 2011.

R. Dutkiewicz and C. A. Hage, “Aspergillus infections in the critically ill,” Proceedings of the American Thoracic Society, vol. 7, no. 3, pp. 204–209, 2010.

A. Glockner and M. Karthaus, “Current aspects of invasive candidiasis and aspergillosis in adult intensive care patients,” Mycoses, vol. 54, pp. 420–433, 2011.

C. Garcia-Vidal, P. Barba, M. Arnan, et al., “Invasive aspergillosis complicating pandemic influenza A, (H1N1) infection in severely immunocompromised patients,” Clinical Infectious Diseases, vol. 53, pp. e16–e19, 2011.

J. Jensen, J. Guinea, M. Torres-Narbona, P. Muñoz, T. Peláez, and E. Bouza, “Post-surgical invasive aspergillosis: an uncommon and under-appreciated entity,” Journal of Infection, vol. 60, no. 2, pp. 162–167, 2010.

A. I. Hidron, M. C. Gongora, A. M. L. Anderson, and C. A. DiazGranados, “Prolonged survival of a patient with AIDS and central nervous system aspergillosis,” Medical Mycology, vol. 47, no. 3, pp. 327–330, 2009.

A. Gupta, M. McKean, S. Haynes et al., “Chronic granulomatous disease presenting as fulminant Aspergillus pneumonitis: a lethal combination?” Pediatric Critical Care Medicine, vol. 10, no. 4, pp. e43–e45, 2009.

J. Lambourne, D. Agranoff, R. Herbrecht et al., “Association of mannose-binding lectin deficiency with acute invasive aspergillosis in immunocompromised patients,” Clinical Infectious Diseases, vol. 49, no. 10, pp. 1486–1491, 2009.

P. Y. Bochud, J. W. Chien, K. A. Marr et al., “Toll-like receptor 4 polymorphisms and aspergillosis in stem-cell transplantation,” The New England Journal of Medicine, vol. 359, no. 17, pp. 1766–1777, 2008.

D. W. Denning and D. A. Stevens, “Antifungal and surgical treatment of invasive aspergillosis: review of 2,121 published cases,” Reviews of Infectious Diseases, vol. 12, no. 6, pp. 1147–1201, 1990.

M. C. Nicolle, T. Benet, A. Thiebaut, et al., “Invasive aspergillosis in patients with hematologic malignancies: incidence and description of 127 cases enrolled in a single institution prospective survey from 2004 to 2009,” Haematologica, vol. 96, pp. 1685–1691, 2011.

F. B. Cakir, E. Cakir, S. G. Berrak et al., “Invasive respiratory aspergillosis is a treatable disease with early diagnosis and aggressive therapy,” Pediatric Hematology and Oncology, vol. 27, no. 6, pp. 422–434, 2010.

M. Michallet, T. Benet, M. Sobh, et al., “Invasive aspergillosis: an important risk factor on the short- and long-term survival of acute myeloid leukemia (AML) patients,” European Journal of Clinical Microbiology & Infectious Diseases, vol. 31, pp. 991–997, 2012.

J. Menzin, J. L. Meyers, M. Friedman et al., “Mortality, length of hospitalization, and costs associated with invasive fungal infections in high-risk patients,” American Journal of Health-System Pharmacy, vol. 66, no. 19, pp. 1711–1717, 2009.

K. B. Tong, C. J. Lau, K. Murtagh, A. J. Layton, and R. Seifeldin, “The economic impact of aspergillosis: analysis of hospital expenditures across patient subgroups,” International Journal of Infectious Diseases, vol. 13, no. 1, pp. 24–36, 2009.

A. Kim, D. P. Nicolau, and J. L. Kuti, “Hospital costs and outcomes among intravenous antifungal therapies for patients with invasive aspergillosis in the United States,” Mycoses, vol. 54, pp. e301–e312, 2011.

L. Y. A. Chai, M. G. Netea, S. Teerenstra et al., “Early proinflammatory cytokines and C-reactive protein trends as predictors of outcome in invasive aspergillosis,” Journal of Infectious Diseases, vol. 202, no. 9, pp. 1454–1462, 2010.

S. C. A. Chen and D. P. Kontoyiannis, “New molecular and surrogate biomarker-based tests in the diagnosis of bacterial and fungal infection in febrile neutropenic patients,” Current Opinion in Infectious Diseases, vol. 23, no. 6, pp. 567–577, 2010.

D. Caillot, J. F. Couaillier, A. Bernard et al., “Increasing volume and changing characteristics of invasive pulmonary aspergillosis on sequential thoracic computed tomography scans in patients with neutropenia,” Journal of Clinical Oncology, vol. 19, no. 1, pp. 253–259, 2001.

R. Greene, “The radiological spectrum of pulmonary aspergillosis,” Medical Mycology, vol. 43, supplement 1, pp. S147–S154, 2005.

A. Hidalgo, R. Parody, R. Martino et al., “Correlation between high-resolution computed tomography and galactomannan antigenemia in adult hematologic patients at risk for invasive aspergillosis,” European Journal of Radiology, vol. 71, no. 1, pp. 55–60, 2009.

N. Kawel, G. M. Schorer, L. Desbiolles, et al., “Discrimination between invasive pulmonary aspergillosis and pulmonary lymphoma using CT,” European Journal of Radiology, vol. 77, pp. 417–425, 2011.

X. S. Li, H. X. Zhu, H. X. Fan, et al., “Pulmonary fungal infections after bone marrow transplantation: the value of high-resolution computed tomography in predicting their etiology,” Chinese Medical Journal, vol. 124, pp. 3249–3254, 2011.

M. Petrik, G. M. Franssen, H. Haas, et al., “Preclinical evaluation of two 68Ga-siderophores as potential radiopharmaceuticals for Aspergillus fumigatus infection imaging,” European Journal of Nuclear Medicine and Molecular Imaging, vol. 39, pp. 1175–1183, 2012.

B. J. A. Rijnders and L. Slobbe, “Bronchoalveolar lavage fluid galactomannan for diagnosis of invasive pulmonary aspergillosis,” Clinical Infectious Diseases, vol. 50, no. 7, pp. 1070–1072, 2010.

A. Paugam, M. T. Baixench, A. Lebuisson, and J. Dupouy-Camet, “Diagnosis of invasive pulmonary aspergillosis: value of bronchoalveolar lavage galactomannan for immunocompromised patients,” Pathologie Biologie, vol. 58, no. 1, pp. 100–103, 2010.

D. W. Denning, S. Park, C. Lass-Florl et al., “High-frequency triazole resistance found in nonculturable aspergillus fumigatus from lungs of patients with chronic fungal disease,” Clinical Infectious Diseases, vol. 52, no. 9, pp. 1123–1129, 2011.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

R. Rüchel and M. Schaffrinski, “Versatile fluorescent staining of fungi in clinical specimens by using the optical brightener Blankophor,” Journal of Clinical Microbiology, vol. 37, no. 8, pp. 2694–2696, 1999.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

D. W. Denning, C. C. Kibbler, and R. A. Barnes, “British Society for Medical Mycology proposed standards of care for patients with invasive fungal infections,” The Lancet Infectious Diseases, vol. 3, no. 4, pp. 230–240, 2003.

J. K. Choi, J. Mauger, and K. L. McGowan, “Immunohistochemical detection of Aspergillus species in pediatric tissue samples,” American Journal of Clinical Pathology, vol. 121, no. 1, pp. 18–25, 2004.

P. J. Paterson, S. Seaton, T. D. McHugh et al., “Validation and clinical application of molecular methods for the identification of molds in tissue,” Clinical Infectious Diseases, vol. 42, no. 1, pp. 51–56, 2006.

J. A. Horvath and S. Dummer, “The use of respiratory-tract cultures in the diagnosis of invasive pulmonary aspergillosis,” American Journal of Medicine, vol. 100, no. 2, pp. 171–178, 1996.

K. L. Mortensen, H. K. Johansen, K. Fuursted, et al., “A prospective survey of Aspergillus spp. in respiratory tract samples: prevalence, clinical impact and antifungal susceptibility,” European Journal of Clinical Microbiology & Infectious Diseases, vol. 30, pp. 1355–1363, 2011.

T. G. M. Bauters and H. J. Nelis, “Rapid and sensitive plate method for detection of Aspergillus fumigatus,” Journal of Clinical Microbiology, vol. 38, no. 10, pp. 3796–3799, 2000.

C. E. Leslie, B. Flannigan, and L. J. R. Milne, “Morphological studies on clinical isolates of Aspergillus fumigatus,” Journal of Medical and Veterinary Mycology, vol. 26, no. 6, pp. 335–341, 1988.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

M. L. Luong, C. J. Clancy, A. Vadnerkar et al., “Comparison of an aspergillus real-time polymerase chain reaction assay with galactomannan testing of bronchoalvelolar lavage fluid for the diagnosis of invasive pulmonary aspergillosis in lung transplant recipients,” Clinical Infectious Diseases, vol. 52, no. 10, pp. 1218–1226, 2011.

A. C. Pasqualotto, M. O. Xavier, L. B. Sánchez et al., “Diagnosis of invasive aspergillosis in lung transplant recipients by detection of galactomannan in the bronchoalveolar lavage fluid,” Transplantation, vol. 90, no. 3, pp. 306–311, 2010.

A. Bergeron, A. Belle, A. Sulahian et al., “Contribution of galactomannan antigen detection in BAL to the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies,” Chest, vol. 137, no. 2, pp. 410–415, 2010.

J. Maertens, V. Maertens, K. Theunissen et al., “Bronchoalveolar lavage fluid galactomannan for the diagnosis of invasive pulmonary aspergillosis in patients with hematologic diseases,” Clinical Infectious Diseases, vol. 49, no. 11, pp. 1688–1693, 2009.

J. Maertens, V. Maertens, K. Theunissen et al., “Bronchoalveolar lavage fluid galactomannan for the diagnosis of invasive pulmonary aspergillosis in patients with hematologic diseases,” Clinical Infectious Diseases, vol. 49, no. 11, pp. 1688–1693, 2009.

E. Fréalle, K. Decrucq, F. Botterel et al., “Diagnosis of invasive aspergillosis using bronchoalveolar lavage in haematology patients: influence of bronchoalveolar lavage human DNA content on real-time PCR performance,” European Journal of Clinical Microbiology and Infectious Diseases, vol. 28, no. 3, pp. 223–232, 2009.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant Recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant Recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant Recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

S. Y. Park, S. O. Lee, S. H. Choi et al., “Aspergillus galactomannan antigen assay in bronchoalveolar lavage fluid for diagnosis of invasive pulmonary aspergillosis,” Journal of Infection, vol. 61, no. 6, pp. 492–498, 2010.

L. Y. Hsu, Y. Ding, J. Phua et al., “Galactomannan testing of bronchoalveolar lavage fluid is useful for diagnosis of invasive pulmonary aspergillosis in hematology patients,” BMC Infectious Diseases, vol. 10, article 44, 2010.

R. Torelli, M. Sanguinetti, A. Moody, et al., “Diagnosis of invasive aspergillosis by a commercial real-time PCR assay for Aspergillus DNA in bronchoalveolar lavage fluid samples from high-risk patients compared to a galactomannan enzyme immunoassay.,” Journal of Clinical Microbiology, vol. 49, pp. 4273–4278, 2011.

R. Torelli, M. Sanguinetti, A. Moody, et al., “Diagnosis of invasive aspergillosis by a commercial real-time PCR assay for Aspergillus DNA in bronchoalveolar lavage fluid samples from high-risk patients compared to a galactomannan enzyme immunoassay,” Journal of Clinical Microbiology, vol. 49, pp. 4273–4278, 2011.

C. Althoff Souza, N. L. Müller, E. Marchiori, D. L. Escuissato, and T. Franquet, “Pulmonary invasive aspergillosis and candidiasis in immunocompromised patients: a comparative study of the high-resolution CT findings,” Journal of Thoracic Imaging, vol. 21, no. 3, pp. 184–189, 2006.

T. J. Walsh, M. C. Wissel, K. J. Grantham, et al., “Molecular detection and species-specific identification of medically important Aspergillus species by real-time PCR in experimental invasive pulmonary aspergillosis,” Journal of Clinical Microbiology, vol. 49, pp. 4150–4157, 2011.

D. Stynen, J. Sarfati, A. Goris et al., “Rat monoclonal antibodies against Aspergillus galactomannan,” Infection and Immunity, vol. 60, no. 6, pp. 2237–2245, 1992.

M. A. S. H. Mennink-Kersten, J. P. Donnelly, and P. E. Verweij, “Detection of circulating galactomannan for the diagnosis and management of invasive aspergillosis,” The Lancet Infectious Diseases, vol. 4, no. 6, pp. 349–357, 2004.

W. Morelle, M. Bernard, J. P. Debeaupuis, M. Buitrago, M. Tabouret, and J. P. Latgé, “Galactomannoproteins of Aspergillus fumigatus,” Eukaryotic Cell, vol. 4, no. 7, pp. 1308–1316, 2005.

K. Y. Yuen, C. M. Chan, K. M. Chan et al., “Characterization of AFMP1: a novel target for serodiagnosis of Aspergillosis,” Journal of Clinical Microbiology, vol. 39, no. 11, pp. 3830–3837, 2001.

M. A. S. H. Mennink-Kersten, J. P. Donnelly, and P. E. Verweij, “Detection of circulating galactomannan for the diagnosis and management of invasive aspergillosis,” The Lancet Infectious Diseases, vol. 4, no. 6, pp. 349–357, 2004.

T. Fontaine, C. Simenel, G. Dubreucq et al., “Molecular organization of the alkali-insoluble fraction of Aspergillus fumigatus cell wall,” The Journal of Biological Chemistry, vol. 275, no. 36, pp. 27594–27607, 2000.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

C. O. Morton, J. Loeffler, A. de Luca et al., “Dynamics of extracellular release of Aspergillus fumigatus DNA and galactomannan during growth in blood and serum,” Journal of Medical Microbiology, vol. 59, no. 4, pp. 408–413, 2010.

M. A. S. H. Mennink-Kersten, J. P. Donnelly, and P. E. Verweij, “Detection of circulating galactomannan for the diagnosis and management of invasive aspergillosis,” The Lancet Infectious Diseases, vol. 4, no. 6, pp. 349–357, 2004.

M. A. Mennink-Kersten, D. Ruegebrink, N. Wasei, et al., “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1, 3-beta-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, pp. 1711–1718, 2006.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

W. W. Hope, M. J. Kruhlak, C. A. Lyman et al., “Pathogenesis of Aspergillus fumigatus and the kinetics of galactomannan in an in vitro model of early invasive pulmonary aspergillosis: implications for antifungal therapy,” Journal of Infectious Diseases, vol. 195, no. 3, pp. 455–466, 2007.

T. Franquet, N. L. Müller, A. Giménez, P. Guembe, J. De La Torre, and S. Bagué, “Spectrum of pulmonary aspergillosis: histologic, clinical, and radiologic findings,” Radiographics, vol. 21, no. 4, pp. 825–837, 2001.

P. E. Verweij, C. M. Weemaes, J. H. A. J. Curfs, S. Bretagne, and J. F. G. M. Meis, “Failure to detect circulating Aspergillus markers in a patient with chronic granulomatous disease and invasive aspergillosis,” Journal of Clinical Microbiology, vol. 38, no. 10, pp. 3900–3901, 2000.

J. E. Bennett, M. M. Friedman, and B. Dupont, “Receptor-mediated clearance of aspergillus, galactomannan,” Journal of Infectious Diseases, vol. 155, no. 5, pp. 1005–1010, 1987.

R. Herbrecht, V. Letscher-Bru, C. Oprea et al., “Aspergillus galactomannan detection in the diagnosis of invasive aspergillosis in cancer patients,” Journal of Clinical Oncology, vol. 20, no. 7, pp. 1898–1906, 2002.

D. Stynen, J. Sarfati, A. Goris et al., “Rat monoclonal antibodies against Aspergillus galactomannan,” Infection and Immunity, vol. 60, no. 6, pp. 2237–2245, 1992.

K. A. Haynes, J. P. Latge, and T. R. Rogers, “Detection of Aspergillus antigens associated with invasive infection,” Journal of Clinical Microbiology, vol. 28, no. 9, pp. 2040–2044, 1990.

D. Stynen, J. Sarfati, A. Goris et al., “Rat monoclonal antibodies against Aspergillus galactomannan,” Infection and Immunity, vol. 60, no. 6, pp. 2237–2245, 1992.

T. R. Rogers, K. A. Haynes, and R. A. Barnes, “Value of antigen detection in predicting invasive pulmonary aspergillosis,” The Lancet, vol. 336, no. 8725, pp. 1210–1213, 1990.

D. Stynen, J. Sarfati, A. Goris et al., “Rat monoclonal antibodies against Aspergillus galactomannan,” Infection and Immunity, vol. 60, no. 6, pp. 2237–2245, 1992.

D. Stynen, J. Sarfati, A. Goris et al., “Rat monoclonal antibodies against Aspergillus galactomannan,” Infection and Immunity, vol. 60, no. 6, pp. 2237–2245, 1992.

R. R. Klont, M. A. S. H. Mennink-Kersten, and P. E. Verweij, “Utility of Aspergillus antigen detection in specimens other than serum specimens,” Clinical Infectious Diseases, vol. 39, no. 10, pp. 1467–1474, 2004.

P. E. Verweij, J. P. Latge, A. J. M. M. Rijs et al., “Comparison of antigen detection and PCR assay using bronchoalveolar lavage fluid for diagnosing invasive pulmonary aspergillosis in patients receiving treatment for hematological malignancies,” Journal of Clinical Microbiology, vol. 33, no. 12, pp. 3150–3153, 1995.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

H. J. Seyfarth, P. Nenoff, J. Winkler, R. Krahl, U. F. Haustein, and J. Schauer, “Aspergillus detection in bronchoscopically acquired material. Significance and interpretation,” Mycoses, vol. 44, no. 9-10, pp. 356–360, 2001.

Z. Racil, I. Kocmanova, M. Toskova, et al., “Galactomannan detection in bronchoalveolar lavage fluid for the diagnosis of invasive aspergillosis in patients with hematological diseases-the role of factors affecting assay performance,” International Journal of Infectious Diseases, vol. 15, pp. e874–e881, 2011.

M. J. Becker, E. J. Lugtenburg, J. J. Cornelissen, C. Van Der Schee, H. C. Hoogsteden, and S. De Marie, “Galactomannan detection in computerized tomography-based broncho-alveolar lavage fluid and serum in haematological patients at risk for invasive pulmonary aspergillosis,” British Journal of Haematology, vol. 121, no. 3, pp. 448–457, 2003.

R. Torelli, M. Sanguinetti, A. Moody, et al., “Diagnosis of invasive aspergillosis by a commercial real-time PCR assay for Aspergillus DNA in bronchoalveolar lavage fluid samples from high-risk patients compared to a galactomannan enzyme immunoassay,” Journal of Clinical Microbiology, vol. 49, pp. 4273–4278, 2011.

P. Danpornprasert, S. Foongladda, and J. Tscheikuna, “Impact of bronchoalveolar lavage galactomannan on the outcome of patients at risk for invasive pulmonary aspergillosis,” Journal of the Medical Association of Thailand, vol. 93, supplement 1, pp. S86–S93, 2010.

S. Y. Park, S. O. Lee, S. H. Choi et al., “Aspergillus galactomannan antigen assay in bronchoalveolar lavage fluid for diagnosis of invasive pulmonary aspergillosis,” Journal of Infection, vol. 61, no. 6, pp. 492–498, 2010.

J. Maertens, V. Maertens, K. Theunissen et al., “Bronchoalveolar lavage fluid galactomannan for the diagnosis of invasive pulmonary aspergillosis in patients with hematologic diseases,” Clinical Infectious Diseases, vol. 49, no. 11, pp. 1688–1693, 2009.

J. Maertens, V. Maertens, K. Theunissen et al., “Bronchoalveolar lavage fluid galactomannan for the diagnosis of invasive pulmonary aspergillosis in patients with hematologic diseases,” Clinical Infectious Diseases, vol. 49, no. 11, pp. 1688–1693, 2009.

M. H. Nguyen, H. Leather, C. J. Clancy et al., “Galactomannan testing in bronchoalveolar lavage fluid facilitates the diagnosis of invasive pulmonary aspergillosis in patients with hematologic malignancies and stem cell transplant Recipients,” Biology of Blood and Marrow Transplantation, vol. 17, no. 7, pp. 1043–1050, 2011.

S. Y. Park, S. O. Lee, S. H. Choi et al., “Aspergillus galactomannan antigen assay in bronchoalveolar lavage fluid for diagnosis of invasive pulmonary aspergillosis,” Journal of Infection, vol. 61, no. 6, pp. 492–498, 2010.

W. Meersseman, K. Lagrou, J. Maertens et al., “Galactomannan in bronchoalveolar lavage fluid: a tool for diagnosing aspergillosis in intensive care unit patients,” American Journal of Respiratory and Critical Care Medicine, vol. 177, no. 1, pp. 27–34, 2008.

J. Acosta, M. Catalan, A. del Palacio-Peréz-Medel et al., “A prospective comparison of galactomannan in bronchoalveolar lavage fluid for the diagnosis of pulmonary invasive aspergillosis in medical patients under intensive care: comparison with the diagnostic performance of galactomannan and of (1→ 3) -β-d-glucan chromogenic assay in serum samples,” Clinical Microbiology and Infection, vol. 17, no. 7, pp. 1053–1060, 2011.

P. E. Verweij, C. M. Weemaes, J. H. A. J. Curfs, S. Bretagne, and J. F. G. M. Meis, “Failure to detect circulating Aspergillus markers in a patient with chronic granulomatous disease and invasive aspergillosis,” Journal of Clinical Microbiology, vol. 38, no. 10, pp. 3900–3901, 2000.

S. I. Kimura, J. Odawara, T. Aoki, M. Yamakura, M. Takeuchi, and K. Matsue, “Detection of sputum Aspergillus galactomannan for diagnosis of invasive pulmonary aspergillosis in haematological patients,” International Journal of Hematology, vol. 90, no. 4, pp. 463–470, 2009.

M. Coates and J. Wilson, “Central nervous system aspergillus infection complicating renal transplantation,” Australasian Radiology, vol. 45, no. 3, pp. 338–342, 2001.

M. Machetti, M. Zotti, L. Veroni et al., “Antigen detection in the diagnosis and management of a patient with probable cerebral aspergillosis treated with voriconazole,” Transplant Infectious Disease, vol. 2, no. 3, pp. 140–144, 2000.

C. Viscoli, M. Machetti, P. Gazzola et al., “Aspergillus galactomannan antigen in the cerebrospinal fluid of bone marrow transplant recipients with probable cerebral aspergillosis,” Journal of Clinical Microbiology, vol. 40, no. 4, pp. 1496–1499, 2002.

M. A. S. H. Mennink-Kersten, J. P. Donnelly, and P. E. Verweij, “Detection of circulating galactomannan for the diagnosis and management of invasive aspergillosis,” The Lancet Infectious Diseases, vol. 4, no. 6, pp. 349–357, 2004.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, R. R. Klont et al., “Improved detection of circulating Aspergillus antigen by use of a modified pretreatment procedure,” Journal of Clinical Microbiology, vol. 46, no. 4, pp. 1391–1397, 2008.

I. Oren, I. Avidor, and H. Sprecher, “Lack of intra-laboratory reproducibility in using Platelia Aspergillus enzyme immunoassay test for detection of Aspergillus galactomannan antigen,” Transplant Infectious Disease, vol. 14, pp. 107–109, 2012.

S. F. Dufresne, K. Datta, X. Li, et al., “Detection of urinary excreted fungal galactomannan-like antigens for diagnosis of invasive Aspergillosis,” PLoS One, vol. 7, Article ID e42736, 2012.

C. M. A. Swanink, J. F. G. M. Meis, A. J. M. M. Rijs, J. P. Donnelly, and P. E. Verweij, “Specificity of a sandwich enzyme-linked immunosorbent assay for detecting Aspergillus galactomannan,” Journal of Clinical Microbiology, vol. 35, no. 1, pp. 257–260, 1997.

M. Mikulska, E. Furfaro, V. Del Bono, et al., “Galactomannan testing might be useful for early diagnosis of fusariosis,” Diagnostic Microbiology and Infectious Disease, vol. 72, pp. 367–369, 2012.

Y. T. Huang, C. C. Hung, and P. R. Hsueh, “Aspergillus galactomannan antigenemia in penicilliosis marneffei,” AIDS, vol. 21, no. 14, pp. 1990–1991, 2007.

P. Vergidis, R. C. Walker, D. R. Kaul, et al., “False-positive Aspergillus galactomannan assay in solid organ transplant recipients with histoplasmosis,” Transplant Infectious Disease, vol. 14, pp. 213–217, 2012.

M. Mikulska, E. Furfaro, B. Del, et al., “Galactomannan testing might be useful for early diagnosis of fusariosis,” Diagnostic Microbiology and Infectious Disease, vol. 72, pp. 367–369, 2012.

A. M. Tortorano, M. C. Esposto, A. Prigitano, et al., “Cross-reactivity of Fusarium spp. in the Aspergillus Galactomannan enzyme-linked immunosorbent assay,” Journal of Clinical Microbiology, vol. 50, pp. 1051–1053, 2012.

F. Dalle, P. E. Charles, K. Blanc et al., “Cryptococcus neoformans galactoxylomannan contains an epitope(s) that is cross-reactive with Aspergillus galactomannan,” Journal of Clinical Microbiology, vol. 43, no. 6, pp. 2929–2931, 2005.

A. Bonini, C. Capatti, M. Parmeggiani et al., “Galactomannan detection in Geotrichum capitatum invasive infections: report of 2 new cases and review of diagnostic options,” Diagnostic Microbiology and Infectious Disease, vol. 62, no. 4, pp. 450–452, 2008.

C. M. A. Swanink, J. F. G. M. Meis, A. J. M. M. Rijs, J. P. Donnelly, and P. E. Verweij, “Specificity of a sandwich enzyme-linked immunosorbent assay for detecting Aspergillus galactomannan,” Journal of Clinical Microbiology, vol. 35, no. 1, pp. 257–260, 1997.

A. Sulahian, S. Touratier, and P. Ribaud, “False positive test for aspergillus antigenemia related to concomitant administration of piperacillin and tazobactam,” The New England Journal of Medicine, vol. 349, no. 24, pp. 2366–2367, 2003.

C. Viscoli, M. Machetti, P. Cappellano et al., “False-positive galactomannan platelia Aspergillus test results for patients receiving piperacillin-tazobactam,” Clinical Infectious Diseases, vol. 38, no. 6, pp. 913–916, 2004.

M. P. Gerlinger, P. Rousselot, S. Rigaudeau, et al., “False positive galactomannan Platelia due to piperacillin-tazobactam,” Médecine et Maladies Infectieuses, vol. 42, pp. 10–14, 2012.

M. Mikulska, E. Furfaro, B. Del, V. Del Bono, et al., “Piperacillin/tazobactam (Tazocin) seems to be no longer responsible for false-positive results of the galactomannan assay,” Journal of Antimicrobial Chemotherapy, vol. 67, pp. 1746–1748, 2012.

L. Millon, F. Grenouillet, J. Crouzet et al., “False-positive Aspergillus real-time PCR assay due to a nutritional supplement in a bone marrow transplant recipient with GVH disease,” Medical Mycology, vol. 48, no. 4, pp. 661–664, 2010.

A. Aceti, L. Corvaglia, and G. Faldella, “Infant formulas thickened with carob bean gum causing false-positive galactomannan test reactivity,” Pediatric Infectious Disease Journal, vol. 27, no. 8, p. 769, 2008.

J. P. Gangneux, D. Lavarde, S. Bretagne, C. Guiguen, and V. Gandemer, “Transient aspergillus antigenaemia: t hink of milk,” The Lancet, vol. 359, no. 9313, p. 1251, 2002.

R. Ansorg, R. van den Boom, and P. M. Rath, “Detection of Aspergillus galactomannan antigen in foods and antibiotics,” Mycoses, vol. 40, no. 9-10, pp. 353–357, 1997.

R. Petraitiene, V. Petraitis, J. R. Witt III, et al., “Galactomannan antigenemia after infusion of gluconate-containing Plasma-Lyte,” Journal of Clinical Microbiology, vol. 49, pp. 4330–4332, 2011.

Z. Racil, I. Kocmanova, M. Lengerova, J. Winterova, and J. Mayer, “Intravenous PLASMA-LYTE as a major cause of false-positive results of platelia Aspergillus test for galactomannan detection in serum,” Journal of Clinical Microbiology, vol. 45, no. 9, pp. 3141–3142, 2007.

C. A. Hage, J. M. Reynolds, M. Durkin, L. J. Wheat, and K. S. Knox, “Plasmalyte as a cause of false-positive results for Aspergillus galactomannan in bronchoalveolar lavage fluid,” Journal of Clinical Microbiology, vol. 45, no. 2, pp. 676–677, 2007.

M. A. S. H. Mennink-Kersten, R. R. Klont, A. Warris, H. J. M. Op Den Camp, and P. E. Verweij, “Bifidobacterium lipoteichoic acid and false ELISA reactivity in aspergillus antigen detection,” The Lancet, vol. 363, no. 9405, pp. 325–327, 2004.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, R. R. Klont et al., “Bifidobacterial lipoglycan as a new cause for false-positive Platelia aspergillus enzyme-linked immunosorbent assay reactivity,” Journal of Clinical Microbiology, vol. 43, no. 8, pp. 3925–3931, 2005.

M. Siemann, M. Koch-Dörfler, and M. Gaude, “False-positive results in premature infants with the Platelia Aspergillus sandwich enzyme-linked immunosorbent assay,” Mycoses, vol. 41, no. 9-10, pp. 373–377, 1998.

P. Rohrlich, J. Sarfati, P. Mariani et al., “Prospective sandwich enzyme-linked immunosorbent assay for serum galactomannan: early predictive value and clinical use in invasive aspergillosis,” Pediatric Infectious Disease Journal, vol. 15, no. 3, pp. 232–237, 1996.

S. H. Armenian, K. A. Nash, N. Kapoor et al., “Prospective monitoring for invasive aspergillosis using galactomannan and polymerase chain reaction in high risk pediatric patients,” Journal of Pediatric Hematology/Oncology, vol. 31, no. 12, pp. 920–926, 2009.

X. Y. Zhang, S. Y. Zhao, and Z. F. Jiang, “Value of serum galactomannan assay in the diagnosis of pediatric invasive pulmonary aspergillosis,” Zhonghua er Ke Za Zhi, vol. 47, no. 2, pp. 83–86, 2009.

E. Castagnola, E. Furfaro, I. Caviglia et al., “Performance of the galactomannan antigen detection test in the diagnosis of invasive aspergillosis in children with cancer or undergoing haemopoietic stem cell transplantation,” Clinical Microbiology and Infection, vol. 16, no. 8, pp. 1197–1203, 2010.

C. D. Pfeiffer, J. P. Fine, and N. Safdar, “Diagnosis of invasive aspergillosis using a galactomannan assay: a meta-analysis,” Clinical Infectious Diseases, vol. 42, no. 10, pp. 1417–1427, 2006.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

M. M. Leeflang, Y. J. Debets-Ossenkopp, C. E. Visser et al., “Galactomannan detection for invasive aspergillosis in immunocompromized patients,” Cochrane Database of Systematic Reviews, no. 4, Article ID CD007394, 2008.

K. A. Marr and W. Leisenring, “Design issues in studies evaluating diagnostic tests for aspergillosis,” Clinical Infectious Diseases, vol. 41, supplement 6, pp. S381–S386, 2005.

W. K. Sun, F. Zhang, X. Y. Xu, et al., “A systematic review of the accuracy of diagnostic test of serum galactomannan antigen detection for invasive aspergillosis,” Zhonghua Jie He He Hu Xi Za Zhi, vol. 33, pp. 758–765, 2010.

C. Mengoli, M. Cruciani, R. A. Barnes, J. Loeffler, and J. P. Donnelly, “Use of PCR for diagnosis of invasive aspergillosis: systematic review and meta-analysis,” The Lancet Infectious Diseases, vol. 9, no. 2, pp. 89–96, 2009.

Y. L. Guo, Y. Q. Chen, K. Wang, S. M. Qin, C. Wu, and J. L. Kong, “Accuracy of BAL galactomannan in diagnosing invasive aspergillosis: a bivariate metaanalysis and systematic review,” Chest, vol. 138, no. 4, pp. 817–824, 2010.

A. Onishi, D. Sugiyama, Y. Kogata, et al., “Diagnostic accuracy of serum 1, 3-beta-D-glucan for pneumocystis jiroveci pneumonia, invasive candidiasis, and invasive aspergillosis: systematic review and meta-analysis,” Journal of Clinical Microbiology, vol. 50, pp. 7–15, 2012.

K. A. Marr, M. Laverdiere, A. Gugel, and W. Leisenring, “Antifungal therapy decreases sensitivity of the Aspergillus galactomannan enzyme immunoassay,” Clinical Infectious Diseases, vol. 40, no. 12, pp. 1762–1769, 2005.

K. A. Marr, M. Laverdiere, A. Gugel, and W. Leisenring, “Antifungal therapy decreases sensitivity of the Aspergillus galactomannan enzyme immunoassay,” Clinical Infectious Diseases, vol. 40, no. 12, pp. 1762–1769, 2005.

M. J. Becker, S. de Marie, M. H. A. M. Fens, H. A. Verbrugh, and I. A. J. M. Bakker-Woudenberg, “Effect of amphotericin B treatment on kinetics of cytokines and parameters of fungal load in neutropenic rats with invasive pulmonary aspergillosis,” Journal of Antimicrobial Chemotherapy, vol. 52, no. 3, pp. 428–434, 2003.

R. M. Winn, A. Warris, P. Gaustad, and T. G. Abrahamsen, “The effect of antifungal agents and human monocytes on in vitro galactomannan release by Aspergillus spp. in liquid culture medium,” Acta Pathologica, Microbiologica, et Immunologica Scandinavica, vol. 115, no. 12, pp. 1364–1369, 2007.

R. Petraitiene, V. Petraitis, A. H. Groll et al., “Antifungal efficacy of caspofungin (MK-0991) in experimental pulmonary aspergillosis in persistently neutropenic rabbits: pharmacokinetics, drug disposition, and relationship to galactomannan antigenemia,” Antimicrobial Agents and Chemotherapy, vol. 46, no. 1, pp. 12–23, 2002.

C. Cordonnier, F. Botterel, R. Ben Amor et al., “Correlation between galactomannan antigen levels in serum and neutrophil counts in haematological patients with invasive aspergillosis,” Clinical Microbiology and Infection, vol. 15, no. 1, pp. 81–86, 2009.

H. He, L. Ding, B. Sun, et al., “Role of galactomannan determinations in bronchoalveolar lavage fluid samples from critically ill patients with chronic obstructive pulmonary disease for the diagnosis of invasive pulmonary aspergillosis: a prospective study,” Critical Care, vol. 16, article R138, 2012.

J. Guinea, M. Torres-Narbona, P. Gijón et al., “Pulmonary aspergillosis in patients with chronic obstructive pulmonary disease: incidence, risk factors, and outcome,” Clinical Microbiology and Infection, vol. 16, no. 7, pp. 870–877, 2010.

S. Husain, E. J. Kwak, A. Obman et al., “Prospective assessment of Platelia Aspergillus galactomannan antigen for the diagnosis of invasive aspergillosis in lung transplant recipients,” American Journal of Transplantation, vol. 4, no. 5, pp. 796–802, 2004.

C. J. Clancy, R. A. Jaber, H. L. Leather et al., “Bronchoalveolar lavage galactomannan in diagnosis of invasive pulmonary aspergillosis among solid-organ transplant recipients,” Journal of Clinical Microbiology, vol. 45, no. 6, pp. 1759–1765, 2007.

P. Tabarsi, A. Soraghi, M. Marjani, et al., “Comparison of serum and bronchoalveolar lavage galactomannan in diagnosing invasive aspergillosis in solid-organ transplant recipients,” Experimental and Clinical Transplantation, vol. 10, pp. 278–281, 2012.

J. Maertens, J. Verhaegen, K. Lagrou, J. Van Eldere, and M. Boogaerts, “Screening for circulating galactomannan as a noninvasive diagnostic tool for invasive aspergillosis in prolonged neutropenic patients and stem cell transplantation recipients: a prospective validation,” Blood, vol. 97, no. 6, pp. 1604–1610, 2001.

F. Suarez, O. Lortholary, S. Buland et al., “Detection of circulating Aspergillus fumigatus DNA by real-time PCR assay of large serum volumes improves early diagnosis of invasive aspergillosis in high-risk adult patients under hematologic surveillance,” Journal of Clinical Microbiology, vol. 46, no. 11, pp. 3772–3777, 2008.

“Anon,” 2012, http://www.bio-rad.com/cmc_upload/Literature/inserts/62794_881051_GB.pdf

W. K. Sun, F. Zhang, X. Y. Xu, et al., “A systematic review of the accuracy of diagnostic test of serum galactomannan antigen detection for invasive aspergillosis,” Zhonghua Jie He He Hu Xi Za Zhi, vol. 33, pp. 758–765, 2010.

M. Zou, L. Tang, S. Zhao, et al., “Systematic review and meta-analysis of detecting galactomannan in bronchoalveolar lavage fluid for diagnosing invasive aspergillosis,” PLoS One, vol. 7, Article ID e43347, 2012.

L. J. Wheat and T. J. Walsh, “Diagnosis of invasive aspergillosis by galactomannan antigenemia detection using an enzyme immunoassay,” European Journal of Clinical Microbiology and Infectious Diseases, vol. 27, no. 4, pp. 245–251, 2008.

J. Salonen, O. P. Lehtonen, M. R. Teräsjärvi, and J. Nikoskelainen, “Aspergillus antigen in serum, urine and bronchoalveolar lavage specimens of neutropenic patients in relation to clinical outcome,” Scandinavian Journal of Infectious Diseases, vol. 32, no. 5, pp. 485–490, 2000.

J. Maertens, V. Maertens, K. Theunissen et al., “Bronchoalveolar lavage fluid galactomannan for the diagnosis of invasive pulmonary aspergillosis in patients with hematologic diseases,” Clinical Infectious Diseases, vol. 49, no. 11, pp. 1688–1693, 2009.

R. Desai, L. A. Ross, and J. A. Hoffman, “The role of bronchoalveolar lavage galactomannan in the diagnosis of pediatric invasive aspergillosis,” Pediatric Infectious Disease Journal, vol. 28, no. 4, pp. 283–286, 2009.

S. Y. Park, S. O. Lee, S. H. Choi et al., “Aspergillus galactomannan antigen assay in bronchoalveolar lavage fluid for diagnosis of invasive pulmonary aspergillosis,” Journal of Infection, vol. 61, no. 6, pp. 492–498, 2010.

J. Maertens, J. Verhaegen, K. Lagrou, J. Van Eldere, and M. Boogaerts, “Screening for circulating galactomannan as a noninvasive diagnostic tool for invasive aspergillosis in prolonged neutropenic patients and stem cell transplantation recipients: a prospective validation,” Blood, vol. 97, no. 6, pp. 1604–1610, 2001.

S. Husain, C. J. Clancy, M. H. Nguyen et al., “Performance characteristics of the platelia Aspergillus enzyme immunoassay for detection of Aspergillus galactomannan antigen in bronchoalveolar lavage fluid,” Clinical and Vaccine Immunology, vol. 15, no. 12, pp. 1760–1763, 2008.

J. P. Latgé, “The cell wall: a carbohydrate armour for the fungal cell,” Molecular Microbiology, vol. 66, no. 2, pp. 279–290, 2007.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

F. M. Marty and S. Koo, “Role of (I → 3)-β-D-glucan in the diagnosis of invasive aspergillosis,” Medical Mycology, vol. 47, supplement 1, pp. S233–S240, 2009.

T. Miyazaki, S. Kohno, K. Mitsutake, S. Maesaki, K. I. Tanaka, and K. Hara, “(1→3)-β-D-glucan in culture fluid of fungi activates factor G, a limulus coagulation factor,” Journal of Clinical Laboratory Analysis, vol. 9, no. 5, pp. 334–339, 1995.

Z. Odabasi, V. L. Paetznick, J. R. Rodriguez, E. Chen, M. R. McGinnis, and L. Ostrosky-Zeichner, “Differences in beta-glucan levels in culture supernatants of a variety of fungi,” Medical Mycology, vol. 44, no. 3, pp. 267–272, 2006.

T. Miyazaki, S. Kohno, K. Mitsutake et al., “Plasma (1→3)-β-D-glucan and fungal antigenemia in patients with candidemia, aspergillosis, and cryptococcosis,” Journal of Clinical Microbiology, vol. 33, no. 12, pp. 3115–3118, 1995.

T. Miyazaki, S. Kohno, H. Koga et al., “G test, a new direct method for diagnosis of candida infection: comparison with assays for beta-glucan and mannan antigen in a rabbit model of systemic candidiasis,” Journal of Clinical Laboratory Analysis, vol. 6, no. 5, pp. 315–318, 1992.

K. Mitsutake, S. Kohno, T. Miyazaki et al., “Detection of (1-3)-β-D-glucan in a rat model of aspergillosis,” Journal of Clinical Laboratory Analysis, vol. 9, no. 2, pp. 119–122, 1995.

T. Obayashi, M. Yoshida, T. Mori et al., “Plasma (1 → 3)-β-D-glucan measurement in diagnosis of invasive deep mycosis and fungal febrile episodes,” The Lancet, vol. 345, no. 8941, pp. 17–20, 1995.

M. Kami, Y. Tanaka, Y. Kanda et al., “Computed tomographic scan of the chest, latex agglutination test and plasma (1→3)-β-D-glucan assay in early diagnosis of invasive pulmonary aspergillosis: a prospective study of 215 patients,” Haematologica, vol. 85, no. 7, pp. 745–752, 2000.

M. Yoshida, T. Obayashi, A. Iwama et al., “Detection of plasma (1 → 3)-β-d-glucan in patients with Fusarium, Trichosporon, Saccharomyces and Acremonium fungaemias,” Medical Mycology, vol. 35, no. 5, pp. 371–374, 1997.

J. W. Pickering, H. W. Sant, C. A. P. Bowles, W. L. Roberts, and G. L. Woods, “Evaluation of a (1→3)-β-D-glucan assay for diagnosis of invasive fungal infections,” Journal of Clinical Microbiology, vol. 43, no. 12, pp. 5957–5962, 2005.

F. M. Marty, S. Koo, J. Bryar, and L. R. Baden, “(1→3)β-D-glucan assay positivity in patients with Pneumocystis (carinii) jiroveci pneumonia,” Annals of Internal Medicine, vol. 147, no. 1, pp. 70–72, 2007.

H. Kanda, K. Kubo, K. Hamasaki et al., “Influence of various hemodialysis membranes on the plasma (1→3)-β-D-glucan level,” Kidney International, vol. 60, no. 1, pp. 319–323, 2001.

M. Ogawa, H. Hori, S. Niiguchi, E. Azuma, and Y. Komada, “False-positive plasma (1→3)-β-D-glucan test following immunoglobulin product replacement in an adult bone marrow recipient,” International Journal of Hematology, vol. 80, no. 1, pp. 97–98, 2004.

M. A. S. H. Mennink-Kersten, A. Warris, and P. E. Verweij, “1,3-β-D-glucan in patients receiving intravenous amoxicillin- clavulanic acid,” The New England Journal of Medicine, vol. 354, no. 26, pp. 2834–2835, 2006.

J. Digby, J. Kalbfleisch, A. Glenn, A. Larsen, W. Browder, and D. Williams, “Serum glucan levels are not specific for presence of fungal infections in intensive care unit patients,” Clinical and Diagnostic Laboratory Immunology, vol. 10, no. 5, pp. 882–885, 2003.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, and P. E. Verweij, “Pseudomonas aeruginosa as a cause of 1,3-β-d-glucan assay reactivity,” Clinical Infectious Diseases, vol. 46, no. 12, pp. 1930–1931, 2008.

Z. Odabasi, G. Mattiuzzi, E. Estey et al., “β-D-glucan as a diagnostic adjunct for invasive fungal infections: validation, cutoff development, and performance in patients with acute myelogenous leukemia and myelodysplastic syndrome,” Clinical Infectious Diseases, vol. 39, no. 2, pp. 199–205, 2004.

L. Senn, J. O. Robinson, S. Schmidt et al., “1,3-β-D-glucan antigenemia for early diagnosis of invasive fungal infections in neutropenic patients with acute leukemia,” Clinical Infectious Diseases, vol. 46, no. 6, pp. 878–885, 2008.

Z. Racil, I. Kocmanova, M. Toskova, et al., “Reactivity of the 1, 3-beta-D-glucan assay during bacteraemia: limited evidence from a prospective study,” Mycoses. In press

G. Metan, K. A. Nedret, C. Agkus, et al., “Can bacteraemia lead to false positive results in 1, 3-beta-d-glucan test? Analysis of 83 bacteraemia episodes in high-risk patients for invasive fungal infections,” Revista Iberoamericana de Micología, vol. 29, pp. 169–171, 2012.

L. Ostrosky-Zeichner, B. D. Alexander, D. H. Kett et al., “Multicenter clinical evaluation of the (1→3) β-D-glucan assay as an aid to diagnosis of fungal infections in humans,” Clinical Infectious Diseases, vol. 41, no. 5, pp. 654–659, 2005.

R. Y. Hachem, D. P. Kontoyiannis, R. F. Chemaly, Y. Jiang, R. Reitzel, and I. Raad, “Utility of galactomannan enzyme immunoassay and (1,3) β-D-Glucan in diagnosis of invasive fungal infections: low sensitivity for aspergillus fumigatus infection in hematologic malignancy patients,” Journal of Clinical Microbiology, vol. 47, no. 1, pp. 129–133, 2009.

P. F. Xu, J. Y. Zhou, H. Zhou, et al., “Serum antigens assay combined with chest CT scan in diagnosis of invasive pulmonary aspergillosisn,” Zhejiang Da Xue Xue Bao Yi Xue Ban, vol. 41, pp. 332–338, 2012.

A. P. Bellanger, F. Grenouillet, T. Henon et al., “Retrospective assessment of β-d-(1,3)-glucan for presumptive diagnosis of fungal infections,” Acta Pathologica, Microbiologica, et Immunologica Scandinavica, vol. 119, no. 4-5, pp. 280–286, 2011.

X. Gao, L. Chen, G. Hu, and H. Mei, “Invasive pulmonary aspergillosis in acute exacerbation of chronic obstructive pulmonary disease and the diagnostic value of combined serological tests,” Annals of Saudi Medicine, vol. 30, no. 3, pp. 193–197, 2010.

M. Lengerova, I. Kocmanova, Z. Racil, et al., “Detection and measurement of fungal burden in a guinea pig model of invasive pulmonary aspergillosis by novel quantitative nested real-time PCR compared with galactomannan and (1, 3)-beta-D-glucan detection,” Journal of Clinical Microbiology, vol. 50, pp. 602–608, 2012.

C. L. Spreadbury, T. Krausz, S. Pervez, and J. Cohen, “Invasive aspergillosis: clinical and pathological features of a new animal model,” Journal of Medical and Veterinary Mycology, vol. 27, no. 1, pp. 5–15, 1989.

C. M. Tang, D. W. Holden, A. Aufauvre-Brown, and J. Cohen, “The detection of Aspergillus spp. by the polymerase chain reaction and its evaluation in bronchoalveolar lavage fluid,” American Review of Respiratory Disease, vol. 148, no. 5, pp. 1313–1317, 1993.

H. Einsele, H. Hebart, G. Roller et al., “Detection and identification of fungal pathogens in blood by using molecular probes,” Journal of Clinical Microbiology, vol. 35, no. 6, pp. 1353–1360, 1997.

L. Klingspor and J. Loeffler, “Aspergillus PCR formidable challenges and progress,” Medical Mycology, vol. 47, supplement 1, pp. S241–S247, 2009.

P. L. White, S. Bretagne, L. Klingspor et al., “Aspergillus PCR: one step closer to standardization,” Journal of Clinical Microbiology, vol. 48, no. 4, pp. 1231–1240, 2010.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

L. Millon, F. Grenouillet, F. Legrand et al., “Ribosomal and mitochondrial DNA target for real-time PCR diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 49, no. 3, pp. 1058–1063, 2011.

W. C. Nierman, A. Pain, M. J. Anderson, et al., “Genomic sequence of the pathogenic and allergenic filamentous fungus Aspergillus fumigatus,” Nature, vol. 438, pp. 1151–1156, 2005.

M. A. S. H. Mennink-Kersten, D. Ruegebrink, N. Wasei, W. J. G. Melchers, and P. E. Verweij, “In vitro release by Aspergillus fumigatus of galactofuranose antigens, 1,3-β-D-glucan, and DNA, surrogate markers used for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 44, no. 5, pp. 1711–1718, 2006.

P. White and A. Barnes, “Polymerase chain reaction (PCR)-based tests,” in Aspergillosis: From Diagnosis To Prevention, A. Pasqualotto, Ed., pp. 135–157, Springer, London, UK, 2010.

S. Perkhofer, B. E. Kehrel, M. P. Dierich et al., “Human platelets attenuate Aspergillus species via granule-dependent mechanisms,” Journal of Infectious Diseases, vol. 198, no. 8, pp. 1243–1246, 2008.

E. C. M. Williamson, J. P. Leeming, H. M. Palmer et al., “Diagnosis of invasive aspergillosis in bone marrow transplant recipients by polymerase chain reaction,” British Journal of Haematology, vol. 108, no. 1, pp. 132–139, 2000.

C. Costa, D. Vidaud, M. Olivi, E. Bart-Delabesse, M. Vidaud, and S. Bretagne, “Development of two real-time quantitative TaqMan PCR assays to detect circulating Aspergillus fumigatus DNA in serum,” Journal of Microbiological Methods, vol. 44, no. 3, pp. 263–269, 2001.

M. E. Bougnoux, C. Dupont, J. Mateo et al., “Serum is more suitable than whole blood for diagnosis of systemic candidiasis by nested PCR,” Journal of Clinical Microbiology, vol. 37, no. 4, pp. 925–930, 1999.

P. L. White, C. Mengoli, S. Bretagne, et al., “Evaluation of Aspergillus PCR protocols for testing serum specimens,” Journal of Clinical Microbiology, vol. 49, pp. 3842–3848, 2011.

E. McCulloch, G. Ramage, B. Jones et al., “Don't throw your blood clots away: use of blood clot may improve sensitivity of PCR diagnosis in invasive aspergillosis,” Journal of Clinical Pathology, vol. 62, no. 6, pp. 539–541, 2009.

J. Loeffler, H. Hebart, U. Brauchle, U. Schumacher, and H. Einsele, “Comparison between plasma and whole blood specimens for detection of Aspergillus DNA by PCR,” Journal of Clinical Microbiology, vol. 38, no. 10, pp. 3830–3833, 2000.

J. Springer, H. Schlossnagel, W. Heinz, et al., “A novel extraction method combining plasma with a whole-blood fraction shows excellent sensitivity and reproducibility for patients at high risk for invasive aspergillosis,” Journal of Clinical Microbiology, vol. 50, pp. 2585–2591, 2012.

M. Hummel, B. Spiess, K. Kentouche et al., “Detection of Aspergillus DNA in cerebrospinal fluid from patients with cerebral aspergillosis by a nested PCR assay,” Journal of Clinical Microbiology, vol. 44, no. 11, pp. 3989–3993, 2006.

T. Vollmer, M. Störmer, K. Kleesiek, and J. Dreier, “Evaluation of novel broad-range real-time PCR assay for rapid detection of human pathogenic fungi in various clinical specimens,” Journal of Clinical Microbiology, vol. 46, no. 6, pp. 1919–1926, 2008.

G. L. Johnson, D. F. Bibby, S. Wong, et al., “A MIQE-compliant real-time PCR assay for Aspergillus detection,” PLoS One, vol. 7, Article ID e40022, 2012.

P. L. White, R. Barton, M. Guiver et al., “A consensus on fungal polymerase chain reaction diagnosis?: A United Kingdom-Ireland evaluation of polymerase chain reaction methods for detection of systemic fungal infections,” Journal of Molecular Diagnostics, vol. 8, no. 3, pp. 376–384, 2006.

D. N. Fredricks, C. Smith, and A. Meier, “Comparison of six DNA extraction methods for recovery of fungal DNA as assessed by quantitative PCR,” Journal of Clinical Microbiology, vol. 43, no. 10, pp. 5122–5128, 2005.

D. Buchheidt, C. Baust, H. Skladny et al., “Detection of Aspergillus species in blood and bronchoalveolar lavage samples from immunocompromised patients by means of 2-step polymerase chain reaction: clinical results,” Clinical Infectious Diseases, vol. 33, no. 4, pp. 428–435, 2001.

J. Loeffler, H. Hebart, R. Bialek et al., “Contaminations occurring in fungal PCR assays,” Journal of Clinical Microbiology, vol. 37, no. 4, pp. 1200–1202, 1999.

L. J. Griffiths, M. Anyim, S. R. Doffman, M. Wilks, M. R. Millar, and S. G. Agrawal, “Comparison of DNA extraction methods for Aspergillus fumigatus using real-time PCR,” Journal of Medical Microbiology, vol. 55, no. 9, pp. 1187–1191, 2006.

J. Springer, J. Loeffler, W. Heinz et al., “Pathogen-specific DNA enrichment does not increase sensitivity of pcr for diagnosis of invasive aspergillosis in neutropenic patients,” Journal of Clinical Microbiology, vol. 49, no. 4, pp. 1267–1273, 2011.

J. Loeffler, K. Kloepfer, H. Hebart et al., “Polymerase chain reaction detection of Aspergillus DNA in experimental models of invasive aspergillosis,” Journal of Infectious Diseases, vol. 185, no. 8, pp. 1203–1206, 2002.

P. L. White, M. D. Perry, J. Loeffler et al., “Critical stages of extracting DNA from Aspergillus fumigatus in whole-blood specimens,” Journal of Clinical Microbiology, vol. 48, no. 10, pp. 3753–3755, 2010.

M. L. Herrera, A. C. Vallor, J. A. Gelfond, T. F. Patterson, and B. L. Wickes, “Strain-dependent variation in 18S ribosomal DNA copy numbers in aspergillus fumigatus,” Journal of Clinical Microbiology, vol. 47, no. 5, pp. 1325–1332, 2009.

L. Klingspor and S. Jalal, “Molecular detection and identification of Candida and Aspergillus spp. from clinical samples using real-time PCR,” Clinical Microbiology and Infection, vol. 12, no. 8, pp. 745–753, 2006.

V. Rickerts, G. Just-Nübling, F. Konrad et al., “Diagnosis of invasive aspergillosis and mucormycosis in immunocompromised patients by seminested PCR assay of tissue samples,” European Journal of Clinical Microbiology and Infectious Diseases, vol. 25, no. 1, pp. 8–13, 2006.

E. Hardak, M. Yigla, I. Avivi, O. Fruchter, H. Sprecher, and I. Oren, “Impact of PCR-based diagnosis of invasive pulmonary aspergillosis on clinical outcome,” Bone Marrow Transplantation, vol. 44, no. 9, pp. 595–599, 2009.

M. Ramírez, C. Castro, J. C. Palomares et al., “Molecular detection and identification of Aspergillus spp. from clinical samples using real-time PCR,” Mycoses, vol. 52, no. 2, pp. 129–134, 2009.

P. L. White, C. J. Linton, M. D. Perry, E. M. Johnson, and R. A. Barnes, “The evolution and evaluation of a whole blood polymerase chain reaction assay for the detection of invasive aspergillosis in hematology patients in a routine clinical setting,” Clinical Infectious Diseases, vol. 42, no. 4, pp. 479–486, 2006.

C. Schabereiter-Gurtner, B. Selitsch, M. L. Rotter, A. M. Hirschl, and B. Willinger, “Development of novel real-time PCR assays for detection and differentiation of eleven medically important Aspergillus and Candida species in clinical specimens,” Journal of Clinical Microbiology, vol. 45, no. 3, pp. 906–914, 2007.

A. Lau, S. Chen, T. Sorrell et al., “Development and clinical application of a panfungal PCR assay to detect and identify Fungal DNA in tissue specimens,” Journal of Clinical Microbiology, vol. 45, no. 2, pp. 380–385, 2007.

L. V. Reddy, A. Kumar, and V. P. Kurup, “Specific amplification of Aspergillus fumigatus DNA by polymerase chain reaction,” Molecular and Cellular Probes, vol. 7, no. 2, pp. 121–126, 1993.

M. Cuenca-Estrella, Y. Meije, C. Diaz-Pedroche et al., “Value of serial quantification of fungal DNA by a real-time PCR-based technique for early diagnosis of invasive aspergillosis in patients with febrile neutropenia,” Journal of Clinical Microbiology, vol. 47, no. 2, pp. 379–384, 2009.

D. W. Denning, S. Park, C. Lass-Florl et al., “High-frequency triazole resistance found in nonculturable aspergillus fumigatus from lungs of patients with chronic fungal disease,” Clinical Infectious Diseases, vol. 52, no. 9, pp. 1123–1129, 2011.

J. W. M. van der Linden, E. Snelders, J. P. Arends, S. M. Daenen, W. J. G. Melchers, and P. E. Verweij, “Rapid diagnosis of azole-resistant aspergillosis by direct PCR using tissue specimens,” Journal of Clinical Microbiology, vol. 48, no. 4, pp. 1478–1480, 2010.

B. Spiess, W. Seifarth, N. Merker, et al., “Development of novel PCR assays to detect azole resistance-mediating mutations of the Aspergillus fumigatus cyp51A gene in primary clinical samples from neutropenic patients,” Antimicrobial Agents and Chemotherapy, vol. 56, pp. 3905–3910, 2012.

J. Loeffler, H. Hebart, P. Cox, N. Flues, U. Schumacher, and H. Einsele, “Nucleic acid sequence-based amplification of Aspergillus RNA in blood samples,” Journal of Clinical Microbiology, vol. 39, no. 4, pp. 1626–1629, 2001.

D. S. Perlin and Y. Zhao, “Molecular diagnostic platforms for detecting Aspergillus,” Medical Mycology, vol. 47, supplement 1, pp. S223–S232, 2009.

C. Park, E. Y. Kwon, N. Y. Shin et al., “Evaluation of nucleic acid sequence based amplification using fluorescence resonance energy transfer (FRET-NASBA) in quantitative detection of Aspergillus 18S rRNA,” Medical Mycology, vol. 49, no. 1, pp. 73–79, 2011.

J. H. Yoo, S. M. Choi, J. H. Choi, E. Y. Kwon, C. Park, and W. S. Shin, “Construction of internal control for the quantitative assay of Aspergillus fumigatus using real-time nucleic acid sequence-based amplification,” Diagnostic Microbiology and Infectious Disease, vol. 60, no. 1, pp. 121–124, 2008.

Y. Zhao, S. Park, P. Warn, R. Shrief, E. Harrison, and D. S. Perlin, “Detection of aspergillus fumigatus in a rat model of invasive pulmonary aspergillosis by real-time nucleic acid sequence-based amplification,” Journal of Clinical Microbiology, vol. 48, no. 4, pp. 1378–1383, 2010.

J. H. Yoo, S. M. Choi, D. G. Lee et al., “Comparison of the real-time nucleic acid sequence-based amplification (RTi-NASBA) with conventional NASBA, and galactomannan assay for the diagnosis of invasive aspergillosis,” Journal of Korean Medical Science, vol. 22, no. 4, pp. 672–676, 2007.

C. O. Morton, L. A. de, L. Romani, et al., “RT-qPCR detection of Aspergillus fumigatus RNA in vitro and in a murine model of invasive aspergillosis utilizing the PAXgene(R) and Tempus RNA stabilization systems,” Medical Mycology, vol. 50, pp. 661–666, 2012.

J. Loeffler, N. Henke, H. Hebart et al., “Quantification of fungal DNA by using fluorescence resonance energy transfer and the Light Cycler system,” Journal of Clinical Microbiology, vol. 38, no. 2, pp. 586–590, 2000.

M. Kami, T. Fukui, S. Ogawa et al., “Use of real-time PCR on blood samples for diagnosis of invasive aspergillosis,” Clinical Infectious Diseases, vol. 33, no. 9, pp. 1504–1512, 2001.

A. S. Pham, J. J. Tarrand, G. S. May, M. S. Lee, D. P. Kontoyiannis, and X. Y. Han, “Diagnosis of invasive mold infection by real-time quantitative PCR,” American Journal of Clinical Pathology, vol. 119, no. 1, pp. 38–44, 2003.

C. Costa, J. M. Costa, C. Desterke, F. Botterel, C. Cordonnier, and S. Bretagne, “Real-time PCR coupled with automated DNA extraction and detection of galactomannan antigen in serum by enzyme-linked immunosorbent assay for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 40, no. 6, pp. 2224–2227, 2002.

C. Halliday, Q. X. Wu, G. James, and T. Sorrell, “Development of a nested qualitative real-time PCR assay to detect Aspergillus species DNA in clinical specimens,” Journal of Clinical Microbiology, vol. 43, no. 10, pp. 5366–5368, 2005.

P. Badiee, A. Alborzi, M. Karimi, et al., “Diagnostic potential of nested PCR, galactomannan EIA, and beta-D-glucan for invasive aspergillosis in pediatric patients,” Journal of Infection in Developing Countries, vol. 6, pp. 352–357, 2012.

J. Faber, N. Moritz, N. Henninger, F. Zepp, and M. Knuf, “Rapid detection of common pathogenic Aspergillus species by a novel real-time PCR approach,” Mycoses, vol. 52, no. 3, pp. 228–233, 2009.

I. Hadrich, C. Mary, F. Makni et al., “Comparison of PCR-ELISA and Real-Time PCR for invasive aspergillosis diagnosis in patients with hematological malignancies,” Medical Mycology, vol. 49, no. 5, pp. 489–494, 2011.

N. Mancini, D. Clerici, R. Diottï et al., “Molecular diagnosis of sepsis in neutropenic patients with haematological malignancies,” Journal of Medical Microbiology, vol. 57, no. 5, pp. 601–604, 2008.

F. Lamoth, K. Jaton, G. Prod'hom et al., “Multiplex blood PCR in combination with blood cultures for improvement of microbiological documentation of infection in febrile neutropenia,” Journal of Clinical Microbiology, vol. 48, no. 10, pp. 3510–3516, 2010.

M. von Lilienfeld-Toal, L. E. Lehmann, A. D. Raadts et al., “Utility of a commercially available multiplex real-time PCR assay to detect bacterial and fungal pathogens in febrile neutropenia,” Journal of Clinical Microbiology, vol. 47, no. 8, pp. 2405–2410, 2009.

J. Steinmann, J. Buer, P. M. Rath, A. Paul, and F. Saner, “Invasive aspergillosis in two liver transplant recipients: diagnosis by SeptiFast: case report,” Transplant Infectious Disease, vol. 11, no. 2, pp. 175–178, 2009.

J. C. Palomares, S. Bernal, M. Marin, et al., “Molecular diagnosis of Aspergillus fumigatus endocarditis,” Diagnostic Microbiology and Infectious Disease, vol. 70, pp. 534–537, 2011.

P. L. White, M. D. Perry, A. Moody, S. A. Follett, G. Morgan, and R. A. Barnes, “Evaluation of analytical and preliminary clinical performance of myconostica mycassay aspergillus when testing serum specimens for diagnosis of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 49, no. 6, pp. 2169–2174, 2011.

R. Torelli, M. Sanguinetti, A. Moody, et al., “Diagnosis of invasive aspergillosis by a commercial real-time PCR assay for Aspergillus DNA in bronchoalveolar lavage fluid samples from high-risk patients compared to a galactomannan enzyme immunoassay,” Journal of Clinical Microbiology, vol. 49, pp. 4273–4278, 2011.

C. Lass-Florl, S. A. Follett, A. Moody, et al., “Detection of Aspergillus in lung and other tissue samples using the MycAssay Aspergillus real-time PCR kit,” Canadian Journal of Microbiology, vol. 57, pp. 765–768, 2011.

C. Halliday, R. Hoile, T. Sorrell et al., “Role of prospective screening of blood for invasive aspergillosis by polymerase chain reaction in febrile neutropenic recipients of haematopoietic stem cell transplants and patients with acute leukaemia,” British Journal of Haematology, vol. 132, no. 4, pp. 478–486, 2006.

R. L. da Silva, P. Ribeiro, N. Abreu et al., “Early diagnosis of invasive aspergillosis in neutropenic patients. comparison between serum galactomannan and polymerase chain reaction,” Clinical Medicine Insights, vol. 4, pp. 81–88, 2010.

S. H. Armenian, K. A. Nash, N. Kapoor et al., “Prospective monitoring for invasive aspergillosis using galactomannan and polymerase chain reaction in high risk pediatric patients,” Journal of Pediatric Hematology/Oncology, vol. 31, no. 12, pp. 920–926, 2009.

M. Hummel, B. Spiess, J. Roder et al., “Detection of Aspergillus DNA by a nested PCR assay is able to improve the diagnosis of invasive aspergillosis in paediatric patients,” Journal of Medical Microbiology, vol. 58, no. 10, pp. 1291–1297, 2009.

W. K. Sun, F. Zhang, X. Y. Xu, et al., “A systematic review of the accuracy of diagnostic test of serum galactomannan antigen detection for invasive aspergillosis,” Zhonghua Jie He He Hu Xi Za Zhi, vol. 33, pp. 758–765, 2010.

M. Reinwald, B. Spiess, W. J. Heinz, et al., “Diagnosing pulmonary aspergillosis in patients with hematological malignancies: a multicenter prospective evaluation of an Aspergillus PCR assay and a galactomannan ELISA in bronchoalveolar lavage samples,” European Journal of Haematology, vol. 89, pp. 120–127, 2012.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

E. McCulloch, G. Ramage, R. Rajendran, et al., “Antifungal treatment affects the laboratory diagnosis of invasive aspergillosis,” Journal of Clinical Pathology, vol. 65, pp. 83–86, 2012.

M. Reinwald, M. Hummel, E. Kovalevskaya, et al., “Therapy with antifungals decreases the diagnostic performance of PCR for diagnosing invasive aspergillosis in bronchoalveolar lavage samples of patients with haematological malignancies,” Journal of Antimicrobial Chemotherapy, vol. 67, pp. 2260–2267, 2012.

M. Hummel, B. Spiess, O. A. Cornely, M. Dittmer, H. Mörz, and D. Buchheidt, “Aspergillus PCR testing: results from a prospective PCR study within the AmBiLoad trial,” European Journal of Haematology, vol. 85, no. 2, pp. 164–169, 2010.

S. H. Armenian, K. A. Nash, N. Kapoor et al., “Prospective monitoring for invasive aspergillosis using galactomannan and polymerase chain reaction in high risk pediatric patients,” Journal of Pediatric Hematology/Oncology, vol. 31, no. 12, pp. 920–926, 2009.

B. Musher, D. Fredricks, W. Leisenring, S. A. Balajee, C. Smith, and K. A. Marr, “Aspergillus galactomannan enzyme immunoassay and quantitative PCR for diagnosis of invasive aspergillosis with bronchoalveolar lavage fluid,” Journal of Clinical Microbiology, vol. 42, no. 12, pp. 5517–5522, 2004.

C. R. Thornton, “Development of an immunochromatographic lateral-flow device for rapid serodiagnosis of invasive aspergillosis,” Clinical and Vaccine Immunology, vol. 15, no. 7, pp. 1095–1105, 2008.

C. Thornton, G. Johnson, and S. Agrawal, “Detection of invasive pulmonary aspergillosis in haematological malignancy patients by using lateral-flow technology,” Journal of Visualized Experiments, vol. 61, article 3721, 2012.

N. P. Wiederhold, C. R. Thornton, L. K. Najvar, W. R. Kirkpatrick, R. Bocanegra, and T. F. Patterson, “Comparison of lateral flow technology and galactomannan and (1→3)-β-D-glucan assays for detection of invasive pulmonary aspergillosis,” Clinical and Vaccine Immunology, vol. 16, no. 12, pp. 1844–1846, 2009.

M. Schütte, P. Thullier, T. Pelat et al., “Identification of a putative Crf splice variant and generation of recombinant antibodies for the specific detection of Aspergillus fumigatus,” PLoS One, vol. 4, no. 8, Article ID e6625, 2009.

W. Hao, Y. X. Pan, Y. Q. Ding et al., “Well-characterized monoclonal antibodies against cell wall antigen of Aspergillus species improve immunoassay specificity and sensitivity,” Clinical and Vaccine Immunology, vol. 15, no. 2, pp. 194–202, 2008.

M. Neustadt, V. Costina, C. Kupfahl et al., “Characterization and identification of proteases secreted by Aspergillus fumigatus using free flow electrophoresis and MS,” Electrophoresis, vol. 30, no. 12, pp. 2142–2150, 2009.

A. Kumar, R. Ahmed, P. K. Singh, and P. K. Shukla, “Identification of virulence factors and diagnostic markers using immunosecretome of Aspergillus fumigatus,” Journal of Proteomics, vol. 74, no. 7, pp. 1104–1112, 2011.

A. Puri, A. Ahmad, and B. P. Panda, “Development of an HPTLC-based diagnostic method for invasive aspergillosis,” Biomedical Chromatography, vol. 24, no. 8, pp. 887–892, 2010.

M. P. Domingo, C. Colmenarejo, L. Martinez-Lostao, et al., “Bis(methyl)gliotoxin proves to be a more stable and reliable marker for invasive aspergillosis than gliotoxin and suitable for use in diagnosis,” Diagnostic Microbiology and Infectious Disease, vol. 73, pp. 57–64, 2012.

R. Kappe and D. Rimek, “Mycoserology did we move on? Aspergillus,” Mycoses, vol. 53, supplement 1, pp. 26–29, 2010.

L. N. Shi, F. Q. Li, J. F. Lu, et al., “Antibody specific to thioredoxin reductase as a new biomarker for serodiagnosis of invasive aspergillosis in non-neutropenic patients,” Clinica Chimica Acta, vol. 413, pp. 938–943, 2012.

J. Sarfati, M. Monod, P. Recco et al., “Recombinant antigens as diagnostic markers for aspergillosis,” Diagnostic Microbiology and Infectious Disease, vol. 55, no. 4, pp. 279–291, 2006.

S. T. Chambers, A. Scott-Thomas, and M. Epton, “Developments in novel breath tests for bacterial and fungal pulmonary infection,” Current Opinion in Pulmonary Medicine, vol. 18, pp. 228–232, 2012.

T. Mahfouz and E. Anaissie, “Prevention of fungal infections in the immunocomprised host,” Current Opinion in Investigational Drugs, vol. 4, no. 8, pp. 974–990, 2003.

P. D. Ziakas, I. S. Kourbeti, E. Mylonakis, and M. Voulgarelis, “Effectiveness of systemic antifungal prophylaxis in patients with neutropenia after chemotherapy: a meta-analysis of randomized controlled trials,” Clinical Therapeutics, vol. 32, no. 14, pp. 2316–2336, 2010.

M. C. Ethier, M. Science, J. Beyene, et al., “Mould-active compared with fluconazole prophylaxis to prevent invasive fungal diseases in cancer patients receiving chemotherapy or haematopoietic stem-cell transplantation: a systematic review and meta-analysis of randomised controlled trials,” British Journal of Cancer, vol. 106, pp. 1626–1637, 2012.

E. D. Ashley, R. Drew, M. Johnson, et al., “Cost of invasive fungal infections in the era of new diagnostics and expanded treatment options,” Pharmacotherapy, vol. 32, pp. 890–901, 2012.

E. Snelders, H. A. L. Van Der Lee, J. Kuijpers et al., “Emergence of azole resistance in Aspergillus fumigatus and spread of a single resistance mechanism,” PLoS Medicine, vol. 5, no. 11, article e219, 2008.

W. T. Hughes, D. Armstrong, G. P. Bodey et al., “2002 Guidelines for the use of antimicrobial agents in neutropenic patients with cancer,” Clinical Infectious Diseases, vol. 34, no. 6, pp. 730–751, 2002.

T. J. Walsh, R. W. Finberg, C. Arndt, et al., “Liposomal amphotericin B for empirical therapy in patients with persistent fever and neutropenia. National Institute of Allergy and Infectious Diseases Mycoses Study Group,” The New England Journal of Medicine, vol. 340, pp. 764–771, 1999.

P. A. Pizzo, K. J. Robichaud, F. A. Gill, and F. G. Witebsky, “Empiric antibiotic and antifungal therapy for cancer patients with prolonged fever and granulocytopenia,” American Journal of Medicine, vol. 72, no. 1, pp. 101–111, 1982.

B. E. De Pauw and J. P. Donnelly, “Timely intervention for invasive fungal disease: should the road now lead to the laboratory instead of the pharmacy?” Clinical Infectious Diseases, vol. 48, no. 8, pp. 1052–1054, 2009.

M. R. Nanda-Rajah, M. A. Slavin, and K. T. Thursky, “The case for antifungal stewardship,” Current Opinion in Infectious Diseases, vol. 25, pp. 107–115, 2012.

C. O. Morrissey, P. G. Bardy, M. A. Slavin et al., “Diagnostic and therapeutic approach to persistent or recurrent fevers of unknown origin in adult stem cell transplantation and haematological malignancy,” Internal Medicine Journal, vol. 38, no. 6, pp. 477–495, 2008.

D. Caillot, O. Casasnovas, A. Bernard et al., “Improved management of invasive pulmonary aspergillosis in neutropenic patients using early thoracic computed tomographic scan and surgery,” Journal of Clinical Oncology, vol. 15, no. 1, pp. 139–147, 1997.

A. Hauggaard, M. Ellis, and L. Ekelund, “Early chest radiography and CT in the diagnosis, management and outcome of invasive pulmonary aspergillosis,” Acta Radiologica, vol. 43, no. 3, pp. 292–298, 2002.

M. Weisser, C. Rausch, A. Droll et al., “Galactomannan does not precede major signs on a pulmonary computerized tomographic scan suggestive of invasive aspergillosis in patients with hematological malignancies,” Clinical Infectious Diseases, vol. 41, no. 8, pp. 1143–1149, 2005.

J. Maertens, K. Theunissen, G. Verhoef et al., “Galactomannan and computed tomography-based preemptive antifungal therapy in neutropenic patients at high risk for invasive fungal infection: a prospective feasibility study,” Clinical Infectious Diseases, vol. 41, no. 9, pp. 1242–1250, 2005.

B. E. de Pauw and C. Viscoli, “Managing invasive fungal infections: relying on clinical instincts or on a rational navigation system?” Journal of Antimicrobial Chemotherapy, vol. 66, supplement 1, pp. i55–i58, 2011.

R. A. Barnes, P. L. White, C. Bygrave, N. Evans, B. Healy, and J. Kell, “Clinical impact of enhanced diagnosis of invasive fungal disease in high-risk haematology and stem cell transplant patients,” Journal of Clinical Pathology, vol. 62, no. 1, pp. 64–69, 2009.

C. Girmenia, A. Micozzi, G. Gentile et al., “Clinically driven diagnostic antifungal approach in neutropenic patients: a prospective feasibility study,” Journal of Clinical Oncology, vol. 28, no. 4, pp. 667–674, 2010.

L. Millon, R. Piarroux, E. Deconinck et al., “Use of real-time PCR to process the first galactomannan-positive serum sample in diagnosing invasive aspergillosis,” Journal of Clinical Microbiology, vol. 43, no. 10, pp. 5097–5101, 2005.

O. Marchetti, F. Lamoth, M. Mikulska, et al., “ECIL recommendations for the use of biological markers for the diagnosis of invasive fungal diseases in leukemic patients and hematopoietic SCT recipients,” Bone Marrow Transplantation, vol. 47, pp. 846–854, 2012.

M. J. Ruping, J. J. Vehreschild, A. Groll, et al., “Current issues in the clinical management of invasive aspergillosis–the AGIHO, DMykG, OGMM and PEG web-based survey and expert consensus conference 2009,” Mycoses, vol. 54, pp. e557–e568, 2011.

J. Maertens, A. H. Groll, C. Cordonnier, R. de la Cámara, E. Roilides, and O. Marchetti, “Treatment and timing in invasive mould disease,” Journal of Antimicrobial Chemotherapy, vol. 66, supplement 1, Article ID dkq440, pp. i37–i43, 2011.

J. Deeks, “Assessing outcomes following tests,” in Evidence-Based Laboratory Medicine, C. Price and R. Christenson, Eds., pp. 95–111, AACC Press, Washington, DC, USA, 2007.

H. Hebart, L. Klingspor, T. Klingebiel et al., “A prospective randomized controlled trial comparing PCR-based and empirical treatment with liposomal amphotericin B in patients after allo-SCT,” Bone Marrow Transplantation, vol. 43, no. 7, pp. 553–561, 2009.

O. Blennow, M. Remberger, L. Klingspor et al., “Randomized PCR-based therapy and risk factors for invasive fungal infection following reduced-intensity conditioning and hematopoietic SCT,” Bone Marrow Transplantation, vol. 45, no. 12, pp. 1710–1718, 2010.

C. Cordonnier, C. Pautas, S. Maury et al., “Empirical versus preemptive antifungal therapy for high-risk, febrile, neutropenic patients: a randomized, controlled trial,” Clinical Infectious Diseases, vol. 48, no. 8, pp. 1042–1051, 2009.

C. O. Morrissey, S. C. A. Chen, T. C. Sorrell et al., “Design issues in a randomized controlled trial of a pre-emptive versus empiric antifungal strategy for invasive aspergillosis in patients with high-risk hematologic malignancies,” Leukemia and Lymphoma, vol. 52, no. 2, pp. 179–193, 2011.

N. Freemantle, P. Tharmanathan, and R. Herbrecht, “Systematic review and mixed treatment comparison of randomized evidence for empirical, pre-emptive and directed treatment strategies for invasive mould disease,” Journal of Antimicrobial Chemotherapy, vol. 66, supplement 1, pp. i25–i35, 2011.

K. A. Marr, “Aspergillus galactomannan index: a surrogate end point to assess outcome of therapy?” Clinical Infectious Diseases, vol. 46, no. 9, pp. 1423–1425, 2008.

J. Maertens, K. Buvé, K. Theunissen et al., “Galactomannan serves as a surrogate endpoint for outcome of pulmonary invasive aspergillosis in neutropenic hematology patients,” Cancer, vol. 115, no. 2, pp. 355–362, 2009.

G. Woods, M. H. Miceli, M. L. Grazziutti, W. Zhao, B. Barlogie, and E. Anaissie, “Serum aspergillus galactomannan antigen values strongly correlate with outcome of invasive aspergillosis: a study of 56 patients with hematologic cancer,” Cancer, vol. 110, no. 4, pp. 830–834, 2007.

A. Bergeron, R. Porcher, J. Menotti, et al., “Prospective evaluation of clinical and biological markers to predict the outcome of invasive pulmonary aspergillosis in hematological patients,” Journal of Clinical Microbiology, vol. 50, pp. 823–830, 2012.

M. H. Miceli, M. L. Grazziutti, G. Woods et al., “Strong correlation between serum aspergillus galactomannan index and outcome of aspergillosis in patients with hematological cancer: clinical and research implications,” Clinical Infectious Diseases, vol. 46, no. 9, pp. 1412–1422, 2008.

S. Koo, J. M. Bryar, L. R. Baden, and F. M. Marty, “Prognostic features of galactomannan antigenemia in galactomannan-positive invasive aspergillosis,” Journal of Clinical Microbiology, vol. 48, no. 4, pp. 1255–1260, 2010.

F. Boutboul, C. Alberti, T. Leblanc et al., “Invasive aspergillosis in allogeneic stem cell transplant recipients: increasing antigenemia is associated with progressive disease,” Clinical Infectious Diseases, vol. 34, no. 7, pp. 939–943, 2002.

O. Penack, P. Rempf, B. Graf, I. W. Blau, and E. Thiel, “Aspergillus galactomannan testing in patients with long-term neutropenia: implications for clinical management,” Annals of Oncology, vol. 19, no. 5, pp. 984–989, 2008.

L. Y. Chai, B. J. Kullberg, E. M. Johnson, et al., “Early serum galactomannan trend as a predictor of outcome of invasive aspergillosis,” Journal of Clinical Microbiology, vol. 50, pp. 2330–2336, 2012.

H. Einsele, K. Quabeck, K. D. Muller et al., “Prediction of invasive pulmonary aspergillosis from colonisation of lower respiratory tract before marrow transplantation,” The Lancet, vol. 352, no. 9138, p. 1443, 1998.

S. H. Kim, C. Park, E. Y. Kwon, et al., “Real-time nucleic acid sequence-based amplification to predict the clinical outcome of invasive aspergillosis,” Journal of Korean Medical Science, vol. 27, pp. 10–15, 2012.

S. Koo, L. R. Baden, and F. M. Marty, “Post-diagnostic kinetics of the (1 →3)-beta-D-glucan assay in invasive aspergillosis, invasive candidiasis and Pneumocystis jirovecii pneumonia,” Clinical Microbiology and Infection, vol. 18, pp. E122–E127, 2012.

V. R. Aquino, F. Nagel, H. F. Andreolla, et al., “The performance of real-time PCR, galactomannan, and fungal culture in the diagnosis of invasive aspergillosis in ventilated patients with chronic obstructive pulmonary disease (COPD),” Mycopathologia, vol. 174, pp. 163–169, 2012.

P. B. De, T. J. Walsh, J. P. Donnelly, et al., “Revised definitions of invasive fungal disease from the European Organization for Research and Treatment of Cancer/Invasive Fungal Infections Cooperative Group and the National Institute of Allergy and Infectious Diseases Mycoses Study Group (EORTC/MSG) Consensus Group,” Clinical Infectious Diseases, vol. 46, pp. 1813–1821, 2008.

N. Azie, D. Neofytos, M. Pfaller, et al., “The PATH (Prospective Antifungal Therapy) Alliance(R) registry and invasive fungal infections: update 2012,” Diagnostic Microbiology and Infectious Disease, vol. 73, pp. 293–300, 2012.

T. Pelaez, P. Munoz, J. Guinea, et al., “Outbreak of invasive aspergillosis after major heart surgery caused by spores in the air of the intensive care unit,” Clinical Infectious Diseases, vol. 54, pp. e24–e31, 2012.

A. Mikolajewska, S. Schwartz, and M. Ruhnke, “Antifungal treatment strategies in patients with haematological diseases or cancer: from prophylaxis to empirical, pre-emptive and targeted therapy,” Mycoses, vol. 55, pp. 2–16, 2012.