BioMed Research International
Volume 2018 (2018), Article ID 1735358, 7 pages
https://doi.org/10.1155/2018/1735358

Research Article

Current Status of Aedes aegypti Insecticide Resistance Development from Banjarmasin, Kalimantan, Indonesia

P. H. Hamid,¹ V. I. Ninditya,¹ J. Prastowo,¹ A. Haryanto,¹ A. Taubert,² and C. Hermosilla²

¹Veterinary Medicine, Gadjah Mada University, Jl. Fauna No. 2, Karangmalang, Yogyakarta, Indonesia
²Institute of Parasitology, Biomedical Research Centre Seltersberg, Justus Liebig University Giessen, Schubertstr. 81, Giessen, Germany

Correspondence should be addressed to P. H. Hamid; penny_hamid@ugm.ac.id

Received 24 June 2018; Revised 2 November 2018; Accepted 5 December 2018; Published 20 December 2018

Academic Editor: Gabriele Gentile

Copyright © 2018 P. H. Hamid et al. 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.

Aedes aegypti represents the principal vector of many arthropod-borne diseases in tropical areas worldwide. Since mosquito control strategies are mainly based on use of insecticides, resistance development can be expected to occur in frequently exposed Ae. aegypti populations. Surveillance on resistance development as well as testing of insecticide susceptibility is therefore mandatory and needs further attention by national/international public health authorities. In accordance, we here conducted a study on Ae. aegypti resistance development towards several often used insecticides, i.e., malathion, deltamethrin, permethrin, λ-cyhalothrin, bendiocarb, and cyfluthrin, in the periurban area of Banjarmasin city, Kalimantan, Indonesia. Our results clearly showed resistance development of Ae. aegypti populations against tested insecticides. Mortalities of Ae. aegypti were less than 90% with the highest resistance observed against 0.75% permethrin. Collected mosquitoes from Banjarmasin also presented high level of resistance development to 0.1% bendiocarb. Molecular analysis of voltage-gated sodium channel (Vgsc) gene showed significant association of V1016G gene point mutation in resistance Ae. aegypti phenotypes against 0.75% permethrin. However, F1534C gene point mutation did not correlate to Ae. aegypti insecticide resistance to 0.75% permethrin. Irrespective of periurban areas in Kalimantan considered as less densed island of Indonesia, Ae. aegypti-derived resistance to different routinely applied insecticides occurred. Our findings evidence that Ae. aegypti insecticide resistance is most likely spreading into less populated areas and thus needs further surveillance in order to delay Ae. aegypti resistance development.

1. Background

Ae. aegypti is the key factor in spreading and transmission of various infectious diseases such as Dengue Fever (DF), Chikungunya, Yellow Fever (YF), and most recently also Zika [1, 2]. Among these viral diseases, DF was classified as most important mosquito-borne disease in the world by WHO due to its wide global burden and associated consequences of economic losses in public health systems [3]. Indonesia is included as “red area” on current WHO risk map for DF together with almost all nations across equator line with tropical/subtropical climates [4]. Due to its large population, Indonesia is the most affected country in South East Asia.

Indonesia is an island chain located in equator which is bridging two continents, namely, Asia and Australia. Our investigated island in this study, Kalimantan or also known as Borneo, has more rural areas than urban/ periurban areas surrounded by wet-rain forest, palm oil plantations, and coal mining companies. Escalating progress of man-made environment influence has resulted in increasing human movements rapidly through modern transportation networks from different islands to less unpopulated islands within Indonesia. History on how Ae. aegypti mosquitoes were introduced and inhabited the island of Kalimantan is still unclear. A feasible scenario of spread by sailors and their ships in colonialism era might have played relevant role in successful colonization of mosquitoes, similar to what happened in the past in Philippines and Hawaii [5]. Since insect control mainly relies on chemical compound usage all over Indonesian archipelago, we evaluated here resistance status of Ae. aegypti populations to frequently insecticides which may reflect changes of ecological bases/habitats in Kalimantan. Current problems faced by Kalimantan are mainly massive deforestation due to expansion of housing areas, extension of new palm oil plantations, coal mining- and logging-activities [6]. Ecological changes in vegetation composition of tropical rain forests, creation of new plantation watering systems, and dam systems for logging economic activities are nowadays considered to have serious impact on epidemiology and spreading of various human vector-borne diseases. Clear example is evidenced by recent ecosystem destruction in Africa where use of dams and culture of rice in paddy-fields produced large expanses of water which are suitable breeding spots for mosquitoes and water snails, both relevant vectors of human diseases such as malaria and schistosomiasis in sub-Saharan Africa [7]. Deforestation is also evidently enhancing landscape becoming warmer and therefore much more hospitable for mosquito colonization [8]. Studies on malaria mosquito vectors evidently showed that deforestation and resulting impact on microclimatic environments greatly influenced life cycles of mosquitoes by reducing vector generation times, increasing reproductive rates, enhancing larval–pupa survival rates, and finally enhancing vector populations [7, 8].

Due to its flexible feeding, as well as breeding habitats, Ae. aegypti has rapidly evolved in last decades as extremely adapted species to human environments. Ae. aegypti’s synanthropic behavior is relatively closer to humans when compared to other Aedes species, e.g., Ae. albopictus, and thus leading to significantly higher spread of Ae. aegypti-transmitted diseases [9]. Reducing Ae. aegypti populations and minimizing interactions with humans are the most reasonable way to control transmitted diseases because complete eradication of suitable vectors and/or viruses is rather unrealistic control approaches [10]. Furthermore, appropriate vaccines and therapies for most human diseases caused by arboviruses are still under development.

Insecticides utilization is considered as the most efficient tools in vector control programs. Insecticide applications can thereby vary from aerosol-space spraying, coils, lotions, clothes, or curtains embedded with certain active insecticide compounds and mass fogging to usage of larvicides in breeding waters. Consequences of national policy breakdown by usage of massive insecticide-based controls with the same active compounds might result in insecticide resistance development. As such, Ae. aegypti resistance development to commonly used insecticides has been reported from different countries worldwide such as Colombia [11], Brazil [12], Grand Cayman [13], Thailand [14], India [15], Malaysia [16], Mexico [17], and China [18]. Consistently to these findings, we previously reported on urban Ae. aegypti resistance development in the cities Denpasar [19] and Jakarta [20] and evidencing increased resistance to commonly used insecticides in Indonesia.

Mechanism of arthropod insecticide resistance development is linked to several pathways which are basically involving metabolic mechanisms and target sites [21]. Main target site for pyrethroid/chlorogenic resistance is represented by mutations in voltage-gated sodium channel (Vgsc) genes of Ae. aegypti [21]. Detailed Vgsc profiling of Aedes has identified at least seven point mutations of insecticide knockdown (kdr) which can clearly lead to reduced sensitivity of arthropod sodium voltage channels to exposed insecticides [22]. Identification of Ae. aegypti specific Vgsc genes showing S989P-, I1011M/V-, V1016G/I-, F1269C-, and F1534C-point mutations is related to this type of resistance [13, 23–26]. At least two of these mutations, i.e., V1016G/I and F1534C, were responsible for pyrethroid resistance as examples in Asia [14, 23, 27] and Latin America [24, 28]. Synergistic resistance may also occur by additional point mutations in different locations of Vgsc genes of Aedes thereby increasing thousands of times resistance capacities mainly towards permethrin-derived insecticides [29].

Kalimantan is well-known endemic area for not only relevant arthropod-borne viral infections, i.e., DF and YF, but also for important arthropod-borne protozoa such as Plasmodium mainly transmitted by endemic Anopheline mosquito species. Chemical compounds of pesticides and insecticides are widely utilized in Kalimantan for several purposes. Such compounds are not only used for controlling malaria and DF vectors, but also for spraying hectares of plantations which is targeting agricultural pest insects. Incidence of resistance development may even occur simultaneously when control programs raised against insects transmitting diseases to humans coincide with control programs against plant pests. Consequently, resistance surveillance has to be performed periodically even in less populated (periurban) or agricultural areas to design strategies for avoiding or minimizing double insecticides exposure of local insect vectors. Although the city centre of Banjarmasin is also containing a relatively dense human population, several urban parts also show less density. Our sampling points were performed in periurban areas of Banjarmasin corresponding to less populated boroughs and further directly bordering forested areas. These sampling sites were in contrast with our previous sampling sites in Denpasar and Jakarta [20, 21], which all were allocated close to the city centre [19, 20]. In this study, we explored resistance development of Ae. aegypti in Banjarmasin, Kalimantan, to several types of commonly used insecticides. Our results provide first important information of current resistance status of Ae. aegypti populations in this investigated area.

2. Methods

2.1. Ethics Approval and Consent to Participate

No ethical clearance was requested as these experiments included exclusively Aedes mosquitoes. Moreover, no mosquito blood feeding was here used and only F0 specimens were used for all experiment settings. The allocation of ovitraps on residential housing areas represented any potential risk of infection neither for humans nor domestic animals and therefore no ethical consent was here issued.

2.2. Mosquito Samples

All mosquitoes in this experiment were collected from periurban areas of the city Banjarmasin (3°19′52.0′′S 114°36′29.3′′E) in South Kalimantan, Indonesia. These collection sites were designed to cover periurban areas of the northern (3°16′23.9′′S 114°35′16.8′′E), southern (3°21′46.0′′S 114°34′55.4′′E), and eastern (3°18′09.9′′S 114°36′42.6′′E) parts of the city. All mosquito samples were collected in July 2017. Ovitraps were placed after obtaining verbal permission from locals as performed in our experiments previously [19, 20]. Briefly, ovitraps were constructed from glass with a black staining outside. A filter paper was placed in the mouth of ovitrap glass and thereafter filled up to 3/4 with tap water. Filled tap water and filter papers were regularly replaced every week during collection dates. Egg-containing filter papers were carefully collected and dried at room temperature (RT), stored, and thereafter transported in plastic containers to the Gadjah Mada University in Yogyakarta, Indonesia. Mosquito eggs were allowed to hatch in the insectary of the Gadjah Mada University. Freshly hatched Ae aegypti-larvae were maintained in plastic containers with tap water daily fed with chicken liver (wet and dried) until reaching adult stage. All adult mosquitoes reared from these collected eggs were thereafter fed with a 10% sugar solution absorbed into cotton balls within specially designed entomological cages of the insectary. Emerged mosquitoes (F0) up to three days old were exclusively used for all insecticide-related experiments.

2.3. Applied Insecticide Susceptibility Tests (ITS)

Insecticide susceptibility tests (IST) were conducted according to the international approved WHO protocols for Anopheline mosquitoes diagnostic doses [30]. Briefly, the kits and insecticide-impregnated filter papers were prepared and supplied by the Vector Control Research Unit, University Sains Malaysia as officially WHO collaborating centre within Southeast Asia. Impregnated filter papers tested were containing 5% malathion, 0.05% deltamethrin, 0.75% permethrin, 0.05%  λ-cyhalothrin, 0.1% bendiocarb, and 0.15% cyfluthrin. In each IST assay, a minimum of 120-150 alive adult mosquitoes from three areas of Banjarmasin were divided into 6 tubes, each containing at least 20-25 mosquitoes. Four tubes (4 replicates) served as replicates for 1 insecticide exposure and two tubes were additionally used as controls. The mosquito mortality was calculated by percentage according to the following formula: total number of dead mosquitoes/total sample size X 100 as reported elsewhere [30]. Abbott’s formula was not used in this study since control mortalities were always less than 5%. The tests were again performed in triplicate. A total number of mosquitoes here tested were 402 specimens for 5% malathion, 404 for 0.05% deltamethrin, 420 for 0.75% permethrin, 402 for 0.05%  λ-cyhalothrin, 420 for 0.1% bendiocarb, and 402 for 0.15% cyfluthrin. Some mosquito survivors as well as dead mosquitoes from these IST bioassays were kept at −20°C for further molecular resistance development analysis. Resistance status of mosquito populations was defined according to the WHO recommendation corresponding to a threshold of < 90% mortality [30].

2.4. DNA Isolation

Isolation of DNA was performed using PureLink® Genomic DNA Isolation Kit (Invitrogen) according to manufacturer instruction. Additionally, we added combination with occasional vortexing using glass beads to ease lysis of mosquitoes in the early step of DNA isolation. Dead and surviving mosquitoes obtained from IST bioassays were extracted individually.

2.5. V1016G and F1534C Genotyping

Genotyping of the mutants V1016G and F1534C was performed according to previous report in literature [14, 31] for allele-specific PCR assays. For detection of V1016G, the PCR consisted of 1 μl of 10 pmol forward primer 5′ACCGACAAATTGTTTCCC3′, 0.5 μl of 10 pmol of each reverse primer 5′GCGGGCAGGGCGGCGGGGGCGGGGCCAGCAAGGCTAAGAAAAGGTTAACTC3′ and 5′GCGGGCAGCAAGGCTAAGAAAAGGTTAATTA3′, 12.5 μl of Dream Taq Green PCR Master Mix® (Thermo Fisher Scientific) in a 25 μl total reaction volume. PCR reactions were performed as follows: 94°C at 2 min, 35 cycles of 30 s at 94°C, 30 s at 55°C, 30 s at 72°C, and a final elongation step for 2 min at 72°C. PCR amplification products were then loaded onto a 3% agarose gel. The F1534C detection PCR consisted of 1 μl of 10 pmol forward primer 5′GCGGGCTCTACTTTGTGTTCTTCATCATATT3′, 0.5 μl of 10 pmol of the forward primer 5′GCGGGCAGGGCGGCGGGGGCGGGGCCTCTACTTTGTGTTCTTCATCATGTG3′ and 1 μl of reverse primer 5′TCTGCTCGTTGAAGTTGTCGAT3′, 12.5 μl of Dream Taq Green PCR Master Mix® (Thermo Fisher Scientific) in a 25 μl total reaction volume. Reactions were performed as follows: 94°C at 2 min, 35 cycles of 30 s at 94°C, 30 s at 60°C, 30 s at 72°C, and a final elongation step for 2 min at 72°C. PCR amplification products were then again loaded onto a 3% agarose gel.

2.6. Statistical Analysis

Statistical analysis and graphical presentation of obtained data were processed by using the commercial available software GraphPad Prism® 7.02. In order to determine mutations associated with resistance, phenotype and odds ratio estimation using recessive model with 95% confidence and Fisher’s exact test were here performed, respectively. Chi square test was performed to evaluate Hardy-Weinberg Equilibrium (HWE). Differences were regarded as significant at the level of P < 0.05.

3. Results

3.1. Adult Ae. aegypti Resistance Development to Tested Insecticides

All adult mosquitoes (n = 2450) reared in laboratory from different locations of Banjarmasin were tested against various insecticides impregnated papers according to WHO protocols [30]. Based on IST results, all Ae. aegypti populations showed various degree of resistance to insecticides with mortalities less than 90% except for malathion 5% (Figure 1). Resistance profiles to permethrin 0.75% and to bendiocarb 0.1% were less than 50% (Figure 1). The highest resistance development observed was against permethrin when compared to any other tested insecticides except bendiocarb 0.1% (0.05% deltamethrin t = 5.059, P < 0.05; 0.05%  λ-cyhalothrin, t = 7.159, P < 0.01; 5% malathion t = 13.63, P < 0.001; 0.1% bendiocarb t = 0.831, P ≥ 0.5; 0.15% cyfluthrin t = 7.42, P < 0.01).

Figure 1: Resistance profiles to different insecticides tested in Ae. aegypti from Banjarmasin, Indonesia, 5% malathion (n= 402), 0.05% deltamethrin (n= 404), 0.75% permethrin (n= 420), 0.05%  λ-cyhalothrin (n= 402), 0.1% bendiocarb (n= 420), and 0.15% cyfluthrin (n= 402). The bars are percentage of mortality after exposure to insecticides with error bars represents standard deviation.

3.2. Mosquito Genotyping of Voltage-Gated Sodium Channel (Vgsc) Gene

PCR genotyping showed distribution of V1016G and F1534C in Vgsc gene domains II and III. In resistant mosquitoes, the wild-type VV homozygotes were 0.14, VG heterozygotes were 0.57, and GG homozygotes were 0.28. In susceptible group, VV frequencies were 0.14, VG were 0.71, and GG were 0.14. Distribution frequencies of total VV, VG, and GG genotypes in Banjarmasin were 0.145, 0.621, and 0.23, respectively. Total V1016 frequency was 0.455 and 1016G was 0.545, respectively (Figure 2(a)). HWE calculation of V1016 and 1016G showed P < 0.05. The descriptive distribution pattern of GG genotype in resistant and susceptible mosquito populations is provided in Table 1. Odd ratio (OR) estimation using recessive model of total GG genotype in V1016G mutations showed significant association (Fisher’s exact test, P = 0.02, OR = 2.33, 95% CI = 1.16-4.59) with permethrin-resistance phenotypes (see Table 1).

Table 1: Association of V1016G and F1534C with resistance to 0.75% permethrin.

type of mutation
phenotypes
genotypes
OR  
(95 CI)
p value of Fisher’s test

VV and VG
GG

V1016G
resistant
109
43

susceptible
71
12
2.33
0.02 (S)

FF and FC
CC
OR  
(95 CI)
p value of fisher’s test

F1534C
resistant
109
3

susceptible
91
2
1.25
1 (NS)

OR= odds ratio.

CI= confidence interval.

S= significant.

NS= nonsignificant.

(a)

(b)

Figure 2: Distribution of V1016G and F1534C of Ae. aegypti in Banjarmasin. (a) VV, VG, GG and FF, FC, CC genotypes frequency.

F1534C distributions of F to C point mutations in Vgsc gene domain III were provided in Figure 2(b). In resistant phenotype, homozygotes frequencies of CC were 0.03 and in heterozygotes FC frequencies were 0.62, respectively. Susceptible mosquito samples showed CC frequencies of 0.02 and of 0.48 for FC frequencies (Figure 2(b)). Distribution frequencies of total FF, FC, and CC genotypes in Banjarmasin were 0.42, 0.56, and 0.02. Total F1534 frequency was 0.698 and 1534C was 0.302 (Figure 2(b)). HWE calculation of F1534 and 1534C showed P < 0.05. The CC genotype was rarely detected in Ae. aegypti populations originating from Banjarmasin. Odd ratio (OR) of F1534C mutation showed no significant association (Fisher’s exact test, P = 1, OR = 1.25, 95% CI = 0.25-7.17) with phenotypes tested against permethrin (Table 1.). Heterozygotes were widely distributed in Ae. aegypti population compared to homozygotes of both wild-type and mutant alleles.

4. Discussion

In contrast with our previous reports from other Indonesian cities [19, 20], Ae. aegypti population in Banjarmasin was still susceptible to 5% malathion since mortality rate achieved more than 90%. Surprisingly, resistance to bendiocarb was as high as for permethrin. The resistance to permethrin is among the highest corroborating previous reports conducted in Indonesia [19, 20, 32, 33]. The genotype frequency of V1016G in Banjarmasin was significantly deviated from HWE. Mosquitoes carrying heterozygote genotype of VG were higher when compared to previous research conducted in Indonesia. The genotype frequency of F1534C in Banjarmasin was also significantly departed from HWE. In accordance with other reports, the CC genotype is found rarely in the mosquito population in Banjarmasin [19, 20, 32, 33]. Considering that knockdown resistance is generally supposed to be a recessive trait [34], we used recessive model to evaluate the association of resistant phenotype with each single point mutation. Molecular analysis of voltage-gated sodium channel (Vgsc) gene showed significant association of V1016G gene point mutation in resistance A. aegypti phenotype against 0.75% permethrin. However, F1534C gene point mutation did not correlate to Ae. aegypti insecticide resistance development to 0.75% permethrin in this experiment.

Our results contribute with additional pivotal data of global development of resistance to insecticides occurring widely worldwide even in islands or geographic areas which were considered less exposed to overuse of insecticides. However, we speculate on possible insecticide cross-use against insects affecting crops and animals. As such, national and international oil palm companies in Kalimantan have used massively agrochemicals in past decades to boost oil production during critical palm culture periods exposed to various insects such as Oryctes spp., Tirathaba spp., Thosea spp., and species of order Lepidoptera. This phenomenon has also been reported in other geographic areas [35] where heavy use of insecticides occurred without selective management and thereby unnecessarily exposing synanthropic insects such as Ae aegypti mosquitoes.

Despite possibilities of insecticide cross-use between crops and animal/human-related insects, mosquito incursion from different areas is now becoming in focus. Several investigations evidently showed that Ae. aegypti can be found in airport entry points and/or seaports [36]. Additionally, wind-blown dispersal of various mosquito species has been demonstrated in the past. Since massive movements of good trades are increasing worldwide, especially by the use of online systems, these might also contribute in mosquito introduction in previously nonendemic areas and should be considered as risk factors by public health authorities. Nowadays everything can be bought via Internet and afterwards delivered with ease by international parcel services from large modern cities to far, less populated and remote areas. This phenomenon needs further attention since changes in trade mechanism through revolution industry 4.0 can not be avoided. Additionally, Ae. aegypti eggs are known to be highly resistant as dried stages and as such to be found in containers of ships crossing long oceanic distances and still surviving for more than a year. This survival strategy of Ae. aegypti allows this species to be transported with ease using global maritime, terrestrial, and air-borne travel and trade networks. Mosquito larvae can hatch easily once eggs become rehydrated in new place and to successfully complete their life cycle. All above-mentioned anthropogenic factors seem significantly to contribute in spread of infectious agents worldwide, crossing political borders, and boundaries. This study in Banjarmasin (Kalimantan/Borneo Island) also showed that distances and geographic barriers, e.g., straits and/or seas can not impede resistance development, as previously demonstrated in our studies in the cities of Denpasar (Bali island) [19] and Jakarta (Java Island) [20]. Another plausible scenario of resistance spread was the recolonization of certain species which occurred for instance in a region declared as being ‘mosquito-free geographic areas/nations’ in Brazil and probably originating from areas in which mosquito eradication was never completely achieved [37]. We stressed the point that control programs have to be nation/international teamworks and furthermore to be coordinated simultaneously between regions across boundaries since insecticide resistance phenotypes/genotypes in a region may be introduced from other islands.

Putting all together, insecticide resistance-related investigations are needed for better understanding molecular based resistance mechanism and to assess resistance status in exposed mosquito populations and helping to reduce overuse of certain insecticides in national control programs. Public health local agencies may also consider combination of biological and nonbiological strategies in controlling these vectors. Additionally, impact of climate and geographic factors (e.g., altitude, temperature, annual precipitation, relative humidity, and biogeographic region) on mosquito-host interactions and spread of these mosquitoes into nonendemic areas of Kalimantan is relevant topics to be considered in future investigations in one of the most biodiversed islands of the planet.

5. Conclusions

Regular surveillance on insecticide resistance development of Ae. aegypti mosquitoes is mandatory to be performed and to cover all main islands of Indonesia to set better goals and allow proper evaluation of on-going mosquito control strategies. It is recommended that insecticide resistance on other disease-transmitting mosquito genera, such as Anopheles and Culex, shall be performed in parallel within this investigated area.

Data Availability

The data used to support the findings of this study are included within the article.

Conflicts of Interest

The authors declare that they have no conflicts of interest. P. H. Hamid, V. I. Ninditya, A. Haryanto, and J. Prastowo performed the experiments, analyzed the data, and was involved in the project administration. P. H. Hamid, C. Hermosilla, and A. Taubert coordinated the work and wrote the manuscript. All authors read and approved the final version of the manuscript.

Acknowledgments

We deeply thank voluntary citizens of Banjarmasin for allowing ovitrap placements in their yards and homes. Experiments of this work were partially supported and financed by DIKTI- (Direktorat Jenderal Pendidikan Tinggi Indonesia-) INSINAS research grant to P. H. Hamid.

References

N. E. A. Murray, M. B. Quam, and A. Wilder-Smith, “Epidemiology of dengue: past, present and future prospects,” Journal of Clinical Epidemiology, vol. 5, no. 1, pp. 299–309, 2013.

G. Benelli and H. Mehlhorn, “Declining malaria, rising of dengue and Zika virus: insights for mosquito vector control,” Parasitology Research, vol. 115, no. 5, pp. 1747–1754, 2016.

WHO, Global Strategy for Dengue Prevention and Control, 2012-2020, WHO Press, Geneva, Switzerland, 2012.

WHO, Dengue, Countries or Areas at Risk, WHO Press, Geneva, Switzerland, 2012.

J. R. Powell and W. J. Tabachnick, “History of domestication and spread of Aedes aegypti--a review,” Memórias do Instituto Oswaldo Cruz, vol. 108, pp. 11–17, 2013.

K. M. Carlson, R. Heilmayr, H. K. Gibbs et al., “Effect of oil palm sustainability certification on deforestation and fire in Indonesia,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 115, no. 1, pp. 121–126, 2018.

E. J. Kweka, E. E. Kimaro, and S. Munga, “Effect of deforestation and land use changes on mosquito productivity and development in western kenya highlands: Implication for malaria risk,” Frontiers in Public Health, vol. 4, p. 238, 2016.

Y. A. Afrane, G. Zhou, B. W. Lawson, A. K. Githeko, and G. Yan, “Effects of microclimatic changes caused by deforestation on the survivorship and reproductive fitness of Anopheles gambiae in western Kenya highlands,” The American Journal of Tropical Medicine and Hygiene, vol. 74, no. 5, pp. 772–778, 2006.

Y. Tsuda, W. Suwonkerd, S. Chawprom, S. Prajakwong, and M. Takagi, “Different spatial distribution of Aedes aegypti and Aedes albopictus along an urban-rural gradient and the relating environmental factors examined in three villages in northern Thailand,” Journal of the American Mosquito Control Association, vol. 22, no. 2, pp. 222–228, 2006.

A. C. Morrison, E. Zielinski-Gutierrez, T. W. Scott, and R. Rosenberg, “Defining challenges and proposing solutions for control of the virus vector Aedes aegypti,” PLoS Medicine, vol. 5, no. 3, p. e68, 2008.

I. Fonseca-González, M. L. Quiñones, A. Lenhart, and W. G. Brogdon, “Insecticide resistance status of Aedes aegypti (L.) from Colombia,” Pest Management Science, vol. 67, no. 4, pp. 430–437, 2011.

E. P. Lima, M. H. S. Paiva, A. P. de Araújo et al., “Insecticide resistance in Aedes aegypti populations from Ceará, Brazil,” Parasites & Vectors, vol. 4, no. 1, p. 5, 2011.

A. F. Harris, S. Rajatileka, and H. Ranson, “Pyrethroid resistance in Aedes aegypti from Grand Cayman,” The American Journal of Tropical Medicine and Hygiene, vol. 83, no. 2, pp. 277–284, 2010.

J. Yanola, P. Somboon, C. Walton, W. Nachaiwieng, P. Somwang, and L.-A. Prapanthadara, “High-throughput assays for detection of the F1534C mutation in the voltage-gated sodium channel gene in permethrin-resistant Aedes aegypti and the distribution of this mutation throughout Thailand,” Tropical Medicine & International Health, vol. 16, no. 4, pp. 501–509, 2011.

R. B. S. Kushwah, C. L. Dykes, N. Kapoor, T. Adak, and O. P. Singh, “Pyrethroid-Resistance and Presence of Two Knockdown Resistance (kdr) Mutations, F1534C and a Novel Mutation T1520I, in Indian Aedes aegypti,” PLOS Neglected Tropical Diseases, vol. 9, no. 1, p. e3332, 2015.

I. H. Ishak, Z. Jaal, H. Ranson, and C. S. Wondji, “Contrasting patterns of insecticide resistance and knockdown resistance (kdr) in the dengue vectors Aedes aegypti and Aedes albopictus from Malaysia,” Parasites & Vectors, vol. 8, no. 1, p. 181, 2015.

G. P. García, A. E. Flores, I. Fernández-Salas et al., “Recent rapid rise of a permethrin knock down resistance allele in Aedes aegypti in México,” PLOS Neglected Tropical Diseases, vol. 3, no. 10, p. e531, 2009.

C.-X. Li, P. E. Kaufman, R.-D. Xue et al., “Relationship between insecticide resistance and kdr mutations in the dengue vector Aedes aegypti in Southern China,” Parasites & Vectors, vol. 8, p. 325, 2015.

P. H. Hamid, J. Prastowo, A. Widyasari, A. Taubert, and C. Hermosilla, “Knockdown resistance (kdr) of the voltage-gated sodium channel gene of Aedes aegypti population in Denpasar, Bali, Indonesia,” Parasites & Vectors, vol. 10, no. 1, 2017.

P. H. Hamid, J. Prastowo, A. Ghiffari, A. Taubert, and C. Hermosilla, “Aedes aegypti resistance development to commonly used insecticides in Jakarta, Indonesia,” PLoS ONE, vol. 12, no. 12, 2017.

J. Hemingway, N. J. Hawkes, L. McCarroll, and H. Ranson, “The molecular basis of insecticide resistance in mosquitoes,” Insect Biochemistry and Molecular Biology, vol. 34, no. 7, pp. 653–665, 2004.

Y. Du, Y. Nomura, G. Satar et al., “Molecular evidence for dual pyrethroid-receptor sites on a mosquito sodium channel,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 110, no. 29, pp. 11785–11790, 2013.

C. Brengues, N. J. Hawkes, F. Chandre et al., “Pyrethroid and DDT cross-resistance in Aedes aegypti is correlated with novel mutations in the voltage-gated sodium channel gene,” Medical and Veterinary Entomology, vol. 17, no. 1, pp. 87–94, 2003.

K. Saavedra-Rodriguez, L. Urdaneta-Marquez, S. Rajatileka et al., “A mutation in the voltage-gated sodium channel gene associated with pyrethroid resistance in Latin American Aedes aegypti,” Insect Molecular Biology, vol. 16, no. 6, pp. 785–798, 2007.

H. Kawada, Y. Higa, O. Komagata et al., “Widespread distribution of a newly found point mutation in voltage-gated sodium channel in pyrethroid-resistant Aedes aegypti populations in Vietnam,” PLOS Neglected Tropical Diseases, vol. 3, no. 10, p. e527, 2009.

R. Srisawat, N. Komalamisra, C. Apiwathnasorn et al., “Field-collected permethrin-resistant Aedes aegypti from central Thailand contain point mutations in the domain IIS6 of the sodium channel gene (kdr),” Southeast Asian Journal of Tropical Medicine and Public Health, vol. 43, no. 6, pp. 1380–1386, 2012.

S. Plernsub, J. Saingamsook, J. Yanola et al., “Additive effect of knockdown resistance mutations, S989P, V1016G and F1534C, in a heterozygous genotype conferring pyrethroid resistance in Aedes aegypti in Thailand,” Parasites & Vectors, vol. 9, no. 1, p. 417, 2016.

L. C. Alvarez, G. Ponce, K. Saavedra-Rodriguez, B. Lopez, and A. E. Flores, “Frequency of V1016I and F1534C mutations in the voltage-gated sodium channel gene in Aedes aegypti in Venezuela,” Pest Management Science, vol. 71, no. 6, pp. 863–869, 2015.

K. Hirata, O. Komagata, K. Itokawa, A. Yamamoto, T. Tomita, and S. Kasai, “A Single Crossing-Over Event in Voltage-Sensitive Na+ Channel Genes May Cause Critical Failure of Dengue Mosquito Control by Insecticides,” PLOS Neglected Tropical Diseases, vol. 8, no. 8, 2014.

WHO, Test procedures for insecticide resistance monitoring in malaria vector mosquitoes, World Health Organization, Geneva, 2013.

S. A. Stenhouse, S. Plernsub, J. Yanola et al., “Detection of the V1016G mutation in the voltage-gated sodium channel gene of Aedes aegypti (Diptera: Culicidae) by allele-specific PCR assay, and its distribution and effect on deltamethrin resistance in Thailand,” Parasites & Vectors, vol. 6, no. 1, p. 253, 2013.

J. R. Wuliandari, S. F. Lee, V. L. White, W. Tantowijoyo, A. A. Hoffmann, and N. M. Endersby-Harshman, “Association between three mutations, F1565C, V1023G and S996P, in the voltage-sensitive sodium channel gene and knockdown resistance in aedes aegypti from yogyakarta, Indonesia,” Insects, vol. 6, no. 3, pp. 658–685, 2015.

S. Sayono, A. P. N. Hidayati, S. Fahri et al., “Distribution of voltage-gated sodium channel (NAV) alleles among the aedes aegypti populations in central Java province and its association with resistance to pyrethroid insecticides,” PLoS ONE, vol. 11, no. 3, p. e0150577, 2016.

T. G. E. Davies, A. O. O'Reilly, L. M. Field, B. A. Wallace, and M. S. Williamson, “Knockdown resistance to DDT and pyrethroids: From target-site mutations to molecular modelling,” Pest Management Science, vol. 64, no. 11, pp. 1126–1130, 2008.

H. A. A. Khan, W. Akram, K. Shehzad, and E. A. Shaalan, “First report of field evolved resistance to agrochemicals in dengue mosquito, Aedes albopictus (Diptera: Culicidae), from Pakistan,” Parasites & Vectors, vol. 4, no. 1, p. 146, 2011.

M.-M. Kuan and F.-Y. Chang, “Airport sentinel surveillance and entry quarantine for dengue infections following a fever screening program in Taiwan,” BMC Infectious Diseases, vol. 12, p. 182, 2012.

P. Kotsakiozi, A. Gloria-Soria, A. Caccone et al., “Tracking the return of Aedes aegypti to Brazil, the major vector of the dengue, chikungunya and Zika viruses,” PLOS Neglected Tropical Diseases, vol. 11, no. 7, p. e0005653, 2017.