African Swine Fever Virus Load in Hematophagous Dipterans Collected in Outbreaks from Romania: Risk Factors and Implications

economic damage. Te summer peaks and river courses have triggered the hypothesis that vectors may be involved in the transmission of the virus. In temperate climates, insect numbers increase in the late summer. Low temperatures and frosts decrease the number of active insects. Teir presence is strongly associated with the nearby wetlands or swamps around the farms. Te aim of our study was to evaluate the risk factors associated with the presence of ASFV DNA in hematophagous dipterans and to analyze the relevance of Ct values obtained following RT-PCR analysis of the positive samples in ASF outbreaks in Romania, as an indication for the viral load. Te current study included 99 pools of stable fies ( Stomoxys calcitrans ) and 296 pools of biting midges ( Culicoides spp.), collected in June-September 2020, from 30 outbreaks of ASF in domestic swine from backyard farms (BF), type A farms (TAF), and commercial farms (CF). All extracted DNA was tested for the presence of the ASFV genome using a real-time PCR protocol. Ct values of 39.53 and below were considered as positive (min: 18.19; median: 31.41; max: 39.53). Te blood meal source was identifed in the hematophagous insects by using a PCR protocol targeting the mitochondrial gene cytochrome c oxidase subunit 1. Data were analyzed using R software v. 4.0.5. In total, 3,158 insects ( S. calcitrans n =198 and Culicoides n =2960) were collected in 23 farms of the 30 outbreak farms. Ten species of biting midges were identifed. Te total number of insect pools showed signifcant diferences according to the month of sampling, with a higher number of pools collected in August and September. Overall, 137 pools out of the 395 examined were positive for the presence of ASFV DNA. Tere was a higher viral DNA load in farms where pigs were present at the moment of sampling compared to farms where pigs were already culled, in S. calcitrans compared to Culicoides spp. and in CF and TAF compared to BF.


Introduction
African swine fever (ASF), caused by the ASF virus (ASFV), is a contagious disease of swine that is associated with a high rate of morbidity, causing hemorrhagic fever-like symptoms and mortality in domestic and wild pigs [1][2][3].Natural vertebrate hosts of the virus in Africa are warthogs (Phacochoerus spp.) and bushpigs (Potamochoerus larvatus), in which infection is unapparent [4].Te virus was introduced from Africa to Europe and South America in the 1950s-1960s.In Spain and Portugal, it remained prevalent for 30 years until eradication.A more recent introduction from Africa to Europe occurred in 2007, when ASFV outbreaks were initially reported in Georgia in the Caucasus region [5].Te frst occurrence of this transboundary disease in the vicinity of Romania was reported in 2012 in Ukraine [6].Since 2014, ASFV has spread across the Baltic States and Poland among wild boars and domestic pigs [7].Moldova notifed the disease as present in September 2016 [8].With the continuous dispersion, the virus has been reported from Czechia and Romania in 2017 and from Hungary in 2018 [9].In August 2018, Bulgaria reported the frst occurrence of the disease on its territory [8].Between 2020 and 2022, 16 European Union (EU) and other non-EU European countries have had reported ASF outbreaks in domestic pigs.Among them are Serbia in January 2020 and Germany, where the ASF entered the country in September 2020 [10].In January 2022, Italy and North Macedonia reported the frst occurrence of the disease.ASF has been eradicated in two European countries: Belgium (eradicated in March 2020) and Czechia (eradicated in April 2018) [10].
In Asia, China was the frst country afected by the ASFV, with the frst cases reported in August 2018.Te disease's spread since 2018 has had a great dispersal among the Asian nations, covering almost the whole continent [8].Since 2005, ASF has been reported in 73 countries throughout the world [10].
ASFV inficted signifcant economic damage on Romania's domestic pig sector.In July 2017, the frst two outbreaks in domestic pigs were confrmed in Satu Mare County, at the border with Ukraine, in northwestern Romania [9].Te frst cases in wild boars were confrmed in Tulcea County, in the southeast of the country, in 2018.Te disease has rapidly spread throughout the country, and by 31 October, 2018, 1,073 outbreaks in domestic pigs and 155 in wild boars had been reported.Romania currently stands out as the country with the highest number of confrmed ASF cases in domestic pigs in Europe.In 2021, the country reported 1,660 outbreaks (with ca.90% of them in domestic pigs), compared to 1,063 in 2020 [11].
Te epidemiology of ASF in Romania initially seemed diferent in comparison to other EU countries, as the majority of outbreaks were reported in domestic pigs and a lower number of cases involved wild boars.Most outbreaks were observed along the Danube River and its major tributaries [9].Interestingly, ASFV also has been introduced into high-security industrial pig farms.Despite the several hypotheses raised, it is not clear yet which is the most common propagation route for the virus into such facilities [12,13].
Considering the number of outbreaks, several studies focused on viral transmission in Romanian pig herds.In backyard farms, wild boar population density, growing crops around the farm, domestic outbreaks within 2 km, short distance to wild boar outbreaks, and professional visits were considered high-risk factors [14].In another study, the presence of water bodies was also found to be an important factor, raising questions regarding waterborne transmission as these waterways nourish backyard properties [15].It has been shown that immediate quarantine stops infection pathways.Afected farms require efective biosecurity protocols [16].
Soft ticks of the genus Ornithodoros have been shown to be competent biological vectors of the ASF virus and are responsible for sporadic spillover of the virus to domestic pigs from the warthog-associated sylvatic cycle in southern and eastern Africa.Here, a cycle involving domestic pigs and similar ticks that live in their shelters has also been described [17].A similar domestic pig-tick cycle involving another Ornithodoros species was responsible for the persistence of infection in the south-western Iberian Peninsula in the last century [18,19].
Te transmission of the virus from the warthog cycle to domestic pigs depends on the Ornithodoros ticks because warthogs do not shed virus and are not able to transmit the virus through direct contact.As explained by Jori and Bastos [20], the ticks are not associated with bushpigs, and any natural contact with the bushpig would be incidental.Anderson et al. [21] demonstrated that experimentally infected bushpigs could transmit the virus to ticks, which could in turn transmit it to pigs, but that hardly constitutes "one of the most important routes of infection" since it is almost impossible that it could happen naturally.Spillover from the warthog-tick cycle to domestic pigs occurs occasionally, but a recent study showed that the vast majority of pig outbreaks in Africa including areas where the warthogtick cycle is present are caused by pigs, people, and fomites and do not involve the ticks at all [22].
Te summer peaks and local association with the presence of river courses have triggered the supposition that other vectors maybe involved in the transmission of ASF virus [23,24].Flying insects show abundance peaks in the warmest period of the year, and especially in the late summer in temperate climates, insect numbers increase.However, the declining autumn temperatures and especially frosts incrementally decrease the number of active insects [25].Insect abundance on farms is also strongly infuenced by the close neighborhood of wetlands, especially the presence of shallow standing water around the pig farms [26].Te frst study, conducted by Mellor et al. in 1987, demonstrated that the stable fy, Stomoxys calcitrans, mechanically transmits ASFV after interrupted feeding, suggesting the putative role of other hematophagous dipterans in ASFV transmission.In addition, under experimental condition, Olesen et al. [27] demonstrated that stable fies that feed on viraemic blood can harbor infective doses of ASFV for at least 12 hours.Te same authors also demonstrated that under experimental conditions that ingestion of infected stable fies by naïve pigs may lead to infection [28].Recently, two independent studies demonstrated that ASFV DNA can be detected in Stomoxys calcitrans and Culicoides spp.collected in ASF outbreaks [29,30].However, so far, there is no clear evidence that the virus is actually transmitted mechanically by such vectors under feld conditions.
ASFV is routinely detected by using a real-time polymerase chain reaction (real-time PCR) [31][32][33][34].Te target DNA is amplifed and identifed in real time by fuorescence emission during the PCR procedure.After several, sequential amplifcation cycles, the amount of fuorescence produced by a PCR reaction tube containing the amplifed DNA target will exceed a predefned level; this number is known as the cycle threshold (Ct) value [35].A Ct value may be used to assess a sample's viral load [36].
Te present manuscript includes data presented in the project report for EFSA [29], completed with a considerable number of insect pools not analyzed therein while performing statistical analysis and using a diferent approach for data interpretation (the inclusion of the quantitative Ct values).Te aim of this study was to systematically evaluate the risk factors associated with the presence of ASFV DNA in hematophagous dipterans and to analyze the relevance of Ct values of the positive samples in ASF outbreaks in Romania as an indication for the viral load.

Samples: Collection and Pooling.
Te current study includes arthropod samples collected in June-September 2020 from 30 outbreaks of ASF in domestic swine from backyard farms (BF) (small, subsistence farms with low levels of biosecurity and producing only for personal consumption), type A farms (TAF) (medium-sized farms with some biosecurity procedures and capable of delivering animals to commercial abattoirs), and commercial farms (CF) (high levels of biosecurity and capable of delivering animals to commercial abattoirs).A set of inclusion criteria that prioritized localities (communes) based on a variety of parameters and a scoring system were used for their selection.All the sampling details, protocols, and methodologies are described in Balmos ¸et al. [29].Literature recommendations were followed to establish the sampling design in case of all these groups.Each farm was sampled once.Five mini CDC UV light traps per farm were used for collecting Culicoides spp.[37].Te traps were placed inside the farms; the collection was conducted during the night.Traps were switched on 1 h before sunset and switched of 1 h after sunrise.
Te trapping method we used for S. calcitrans was based on sticky traps, commercial traps known as Knight Stick.On each farm, two diferent locations were chosen.Te traps were placed outside, near the animals, at a distance of maximum 15 m and at 1.6 m height.Te collection was conducted during the daylight, as stable fies are active during the day and attracted to translucent or blue-coloured objects.All stable fies and biting midges were preserved in 70% ethanol and kept at −20 °C prior to morphological identifcation and testing for ASFV DNA presence and blood meal source.From all the collected arthropods, only stable fies (Stomoxys calcitrans) and biting midges (Culicoides spp.) were included in the current analysis.Te identifcation of arthropods was based on morphological characteristics, using keys and descriptions [38,39].
Pools were made prior to DNA extraction.Pooling was conducted based on the insect species, collection date, and farm.Due to size diferences among insect groups, stable fies were tested in pools of 2 insects per pool and biting midges in 10 insects per pool, as previously suggested [40,41].Pools were only created if the minimum number of insects per pool (2 or 10) was available.
Te 395 pools (99 for S. calcitrans and 296 for Culicoides spp.) included in the current study are detailed in Table 1.

Real-Time PCR.
All extracted DNA was tested for the presence of the ASFV genome at the National Reference Laboratory (IDAH-Institute for Diagnosis and Animal Health) using a real-time PCR protocol, according to Standard Operating Procedure (SOP) Identifcation of the ASFV genome based on the European Union Reference Laboratory for African Swine Fever (ASF EURL) SOPs [33].DNA extraction was performed at IDAH, individually from each pool, according to the same SOPs.
Pooled samples were ground in MagNa Lyser Green Beads with 1.5 ml cold phosphate bufered saline (PBS1x) supplemented with 0.1% of antibiotic (gentamicin sulphate).Suspensions were clarifed by centrifugation at 5,000 g during 5 min, and 200 μl supernatant was used immediately for ASFV genome detection or stored at <−70 °C until further use.
A Ct value was obtained for each positive sample.Tis value indirectly characterizes the viral load, by providing quantitative data for the amount of ASFV DNA.For this study, we considered samples with Ct values of 39.53 and below as positive.

Identifcation of the Blood Meal
Source.Blood meal analysis was conducted in order to evaluate if the vectors feed on pigs or on other hosts and to check if the ASFV DNA positive vectors have fed on pigs.However, our method is not able to distinguish between wild and domestic pigs.Nevertheless, wild boars were not present at the site of vector sampling during our work.Te PCR amplifcation targeted the cytochrome c oxidase subunit 1 (COI) gene region (∼758 bp).Te reaction was performed in 25 μl total volume, containing 12.5 μl MyTaq ™ Red Mix (Meridian, Teltow, Germany), 6.5 μl of ultrapure water, 1 μl (10 pmol/μL) of each of the two primers M13BCV-FW (5′-TGT AAA ACG ACG GCC AGT HAA YCA YAA RGA YAT YGG -3′) and BCV-RV1 (5′-GCY CAN ACY ATN CCY ATR T -3′) [42], and 4 μl aliquot of the previously isolated DNA.One negative control consisting inultra-pure water was included.Te PCR reaction was performed using the T1000 ™ Termal Cycler (Bio-Rad, London, UK) with the following conditions: initial denaturation at 95 °C for 2 min, followed by 35 cycles of denaturation at 95 °C for 1 min, annealing at 45 °C for 1 min, and extension at 72 °C for 1 min, with a fnal extension at 72 °C for 5 min.Te frst PCR amplifcation was followed by a second reaction (nested PCR) performed in Transboundary and Emerging Diseases 25 μl total volume, containing 12.5 μl Red PCR Mastermix (Rovalab GmBH, Teltow, Germany), 8.5 μl of ultrapure water, 1 μl (10 pmol/μL) of each of the two primers M13 (5′-TGT AAA ACG ACG GCC AGT -3′) and BCV-RV2 (5′-ACY ATN CCY ATR TAN CCR AAN GG -3′) [42], and 2 μl of the initial PCR reaction mix.A second negative control consisting in ultrapure water was included.Te second amplifcation (nested PCR) was performed with the following conditions: initial denaturation at 95 °C for 2 min, denaturation at 95 °C for 1 min, followed by 15 cycles of a touch down protocol decreasing the annealing temperature from 60 °C to 45 °C for 1 min (−1 °C/cycle), and extension at 72 °C for 1 min, followed by another 25 cycles of initial denaturation at 95 °C for 2 min, denaturation at 95 °C for 1 min, annealing at 45 °C for 1, and extension at 72 °C for 1 min, with a fnal extension at 72 °C for 5 min.
Te amplifed products were visualized by the use of electrophoresis on 1.5% agarose gel stained with ECO Safe 20,000× Nucleic Acid Staining Solution (Pacifc Image Electronics, New Taipei, Taiwan), and their molecular weight was compared to a molecular marker (O'GeneRuler ™ 100 bp DNA Ladder, Termo Fisher Scientifc Inc., Waltham, MA, USA).All positive PCR products were purifed using the ISOLATE II PCR and Gel Kit (Bioline Meridian Bioscience, Luckenwalde Germany) and sequenced by the use of an external service (Macrogen Europe, Amsterdam, the Netherlands).All positive sequences were compared with those available in GenBank ™ by the use of Basic Local Alignments Tool (BLAST) analyses.All positive sequences were analyzed and edited by the use of Geneious ® 4.85   software [43].

Statistical Analysis and
Mapping.Data were analyzed using R software v. 4.0.5.Te Shapiro-Wilkinson normality test was used to evaluate the distribution of numerical data.Te observed prevalence of infection related to each category and its 95 confdence interval (95% CI; Wald confdence interval) were calculated.Statistical associations between diferent categorical variables were assessed using Pearson's chi-squared and chi-square goodness of ft tests.Te relationship between the month of sampling, farm type, presence/absence of pigs at the moment of sampling, presence/absence of pig DNA in the vector pool, and insect species on one side and Ct values on the other side was evaluated by the Mann-Whitney U test and Kruskal-Wallis rank sum test.To test for colinearity and combined efects of multiple predictors, we ran a logistic regression, where farm location was included as a random efect.Ct values were considered both as quantitative variables and categorical data when classifed based on the positivity degree (>30 weakly positive, 30-24 positive, and <24 strongly positive).Te phi (Φ) coefcient was used to analyze the strength of association between the presence/absence of pigs or the insect genus and the presence of ASFV.Results were considered statistically signifcant at a P value< 0.05.Te maps were generated using QGis 3.6.2software (https://www.qgis.org).

Collected Arthropods.
In total, 3,158 insects (Stomoxys calcitrans n � 198 and Culicoides n � 2960) were collected in 23 outbreak farms out of the 30 sampled farms (in 7 farms, no Stomoxys or Culicoides were collected).Tese resulted in a total number of 395 pools.Based on the morphological characteristics, 10 species of biting midges were identifed, divided into 296 pools (Table 2).Te stable fies collected were all identifed as Stomoxys calcitrans (Table 3).Te number of insects per pool is shown in "Supplementary fle 1_Number of insects per each pool." Te total number of insect pools showed signifcant diferences according to the month of sampling, with a higher number of pools collected in August and September (X 2 � 262.51, d.f.� 3, and P < 0.001).Te total number of Culicoides pools was signifcantly higher in August and September, when compared to July (X 2 � 242.92, d.f.� 3, and P < 0.001).Moreover, a higher number of Culicoides obsoletus (X 2 � 391.09, d.f.� 9, and P < 0.01) was observed when compared to the other Culicoides spp.Te total number of S. calcitrans pools was higher in August when compared to the other months of sampling (X 2 � 84.636, d.f.� 3, and P < 0.01).

Transboundary and Emerging Diseases
Tere was a statistically signifcant correlation between the overall prevalence of ASFV DNA positive pools according to the month of sampling (X 2 � 41.969, d.f.� 3, and P < 0.001), with the highest prevalence in August.A lower rate of infection was observed in case of BF and TAF, when compared to cu CF (X 2 � 106.22,d.f.� 2, and P < 0.001 ).A statistically signifcant correlation was also identifed between positive ASFV DNA pools and the insect group (Culicoides spp. vs. S. calcitrans) (X 2 � 33.318, d.f.� 1, and P < 0.001) with higher rates recorded in Stomoxys calcitrans (fair positive correlation; Φ � 0.29).
Te prevalence of ASFV DNA positive pools was signifcantly higher (X 2 � 94.003, d.f.� 1, and P < 0.001) in farms where sampling was performed when pigs were still present (60.45%,95% CI: 53.25-67.66)compared to farms where pigs were already culled by the time of sampling (13.76%, 95% CI: 9. 19-18.33).Tere was a moderate correlation (Φ � −0.49) between the presence of ASFV DNA positive pools and the presence of living pigs.However, only pig absence/presence (Z < 0.001) and the month of sampling (Z � 0.1998) were retained as signifcant predictors of ASF DNA positivity, when the combined efect of multiple predictors was tested (logistic regression, farm location used as a random efect).
Out of 395 pools, 51 (12.91%; 95% CI: 9.60-16.22)contained vertebrate DNA, pig DNA detected in 37 pools (9.37%; 95% CI: 6.49-12.24).Pig DNA was detected only in vectors collected in August from two CF farms where pigs were still present at the time of sampling and one TAF where the pigs were already culled at the time of sampling.Pig DNA was detected in four species of vectors: C. obsoletus, C. punctatus, C. pulicaris, and Stomoxys calcitrans.However, no statistically signifcant diferences were noticed between species.
All pools positive for pig DNA were also positive for ASFV DNA.From the pools negative for pig DNA, 19.43% were positive in the case of Culicoides and 55.91% for S. calcitrans.

ASFV DNA Ct Values.
Obtained CT values of the positive samples ranged from 18.19 to 39.53, with a median value of 31.41 and a mean value of 30.14.When Ct values (as quantitative data) were correlated with the presence or absence of pigs, signifcantly lower Ct values (corresponding to higher viral DNA load) were obtained in farms where pigs were present during sampling (Mann-Whitney U test, W � 2599.5, and P < 0.001).
Moreover, when the categorical data were taken into consideration, the absence of pigs in the farms was statistically associated with a higher number of weak results and no strongly positive results were obtained (Pearson's chisquare test, X 2 � 15.966, d.f.� 2, and P < 0.001).
Regarding the insect group (Culicoides spp.and S. calcitrans), signifcantly lower Ct values were obtained in S. calcitrans than in Culicoides spp., meaning a higher viral DNA load in the previous one (Mann-Whitney U-test, W � 3042, and P � 0.001).
Strongly positive Ct values (as categorical data) were signifcantly more common in S. calcitrans than in Culicoides spp.(Pearson's chi-square test, X 2 � 43.732, d.f.� 2, and P < 0.001).while in TAF and CF, positive and strongly positive results were predominant.Te results are considered statistically signifcant with a P value of 0.03 (X 2 � 11.057, d.f.� 4).A signifcantly higher number of strongly positive pools (Ct values below 24) were noticed in June, while weak results (Ct values above 30) were predominant in pools from September (Pearson's chi-square test, X 2 � 25.342, d.f.� 6, and P < 0.001).
Te Kruskal-Wallis test was performed in order to perform the correlation between Ct values categories and the sampling month of the insects.No statistically signifcant results were obtained.
Moreover, no signifcant association was identifed between the three categories of Ct values and the presence of pig DNA.

Discussion
Te presence of ASFV DNA in hematophagous insects was demonstrated on several occasions, under experimental [27,28,44] or feld conditions [29,30].Understanding the risk factors associated with the presence of ASFV DNA in hematophagous insects which are demonstrated as mechanical vectors for other diseases (i.e., Culicoides, Stomoxys) represents the basis for such complex experimental studies.
Tis was experimentally demonstrated for ASFV by S. calcitrans [44].Biting midges can transmit a variety of arboviruses because of their recurring need for blood meals [45].Culicoides ecology, their presence in pig farms [46,47], and ability to mechanically transmit pathogens make them potential vectors for ASFV mechanical transmission.Culicoides spp.are able to feed on pigs [48].Although they ingest very small quantities of blood (approx. 1 μl) and get very low viral doses from infected animals, their abundant presence may facilitate mechanical transmission and infection of healthy animals due to frequent bites and injection of sufcient viral doses.Moreover, in the eventuality of infection, their high capacity for passive dispersal may contribute to virus transmission [24].However, no studies have been conducted to assess if Culicoides spp.can transmit ASF.
In a recent study from Lithuania, Turčinavičienė et al. [30] [53], using the same quantitative approach to identify ASFV DNA, obtained negative results in more than 400 mosquitoes sampled from fve ASF outbreaks in China.Up to date, the involvement of S. calcitrans or Culicoides spp. in the mechanical transmission of ASFV has never been demonstrated under feld conditions.Our study is the frst one to evaluate indirectly the viral load (by assessing the Ct values) in stable fies and biting midges collected from ASF outbreaks and to evaluate the risk factors associated with the viral DNA presence and quantity in these insects.Our study demonstrated that there is a higher viral DNA load in (1) farms where pigs were present at the moment of sampling compared to farms were pigs were already culled; (2) S. calcitrans compared to Culicoides spp.; (3) CF and TAF compared to BF.
Additionally, we demonstrated that the possibility of fnding ASFV DNA in hematophagous dipterans collected from ASF outbreaks is higher in (1) commercial farms compared with other types of farms; (2) farms where pigs are still present at the time of sampling; (3) insects collected during August; (4) Stomoxys compared with Culicoides.Te possibility of fnding pig DNA in hematophagous dipterans blood meal collected from ASF outbreaks was higher in (1) vectors collected in farms where pigs were present at the moment of sampling; (2) ASFV DNA positive samples; (3) August compared to June, July, or September.
Both Culicoides and Stomoxys are able to take their blood meal on a variety of host species, which are more available in a BF than in a CF or TAF.Moreover, at least for Stomoxys, an individual insect can feed on multiple hosts before being fully engorged.Hypothetically, another element could contribute in contradiction with an interesting hypothesis: ASF-afected pigs could be preferred feeding hosts due to their impaired mobility due to disease.
An accurate understanding of the novel mechanical ASFV vectors is important because it could give a better idea of how this virus can be spread, making it easier to control outbreaks and protect pig farms, among other diseases as well.
In conclusion, our data bring new evidence for the possible role of S. calcitrans and Culicoides spp. as mechanical vectors for ASFV, highlighting the risk associated with higher viral loads which could improve the approach to the prevention and control, mainly in commercial farms through a better management of biting insects [54].

Data Availability
All supporting data are available in the current study or can be accessed upon a request from the corresponding author.

Figure 1 :Figure 2 :
Figure 1: Te distribution of sampling sites for Culicoides spp.and the positivity to ASF DNA.

Table 1 :
Pools of S. calcitrans and Culicoides spp.used for this study.

Table 2 :
Number of pools of Culicoides per species by the month of collection, type of farm (CF � commercial farm; TAF � type A farm; BF � backyard farm), and presence of pigs at the time of sampling.

Table 3 :
Number of localities and pools where Stomoxys calcitrans was sampled.
[51]rted the presence of ASF DNA in Stomoxys calcitrans, Culicidae, Calliphoridae, and other Muscidae, but no correlation of Ct values was performed, and no risk factors were analyzed.Similar qualitative data are available from Poland, where ASFV DNA was detected in S. calcitrans Mazur-Panasiuk et al., unpublished data in[49].Herm et al.[12]demonstrated the presence of ASFV DNA in fies (Musca domestica, Drosophila spp.) and mosquitoes collected in ASF outbreaks in Estonia; however, high Ct values were obtained.In addition, Forth et al.[50]demonstrated the presence of ASFV DNA in two blowfy species larvae under experimental conditions, however without isolating infectious virus.Other feld studies did not identify ASF DNA in hematophagous or other arthropods.Yoon et al.[51]reported no traces of ASFV DNA in a large sample set of arthropods