Pyrethroid and DDT resistance and organophosphate susceptibility among Anopheles spp. mosquitoes, Western Kenya.
During April 2012-July 2013, we conducted this study in 7 sentinel sites across different malaria-endemic zones in western Kenya (Figure 1). Malaria vector dynamics and parasite prevalence have been studied in 3 sites (9), and ITN coverage was generally >80% (10). Bungoma, Emutete, Iguhu, and Emakakha are in the highland-fringe malaria epidemic area; Chulaimbo, Ahero, and Kisian are in the malaria-endemic basin region of Lake Victoria (lowland). All sample sites were in rural or suburban areas.
Agricultural and public health use of insecticides in each study site was surveyed by using questionnaire surveys in 30 randomly selected households per site. Mosquito larvae were collected from each study site, fed with TetraMin fish food (Spectrum Brands, Inc., Blacksburg, VA, USA), and raised to adults in the insectary at the Kenya Medical Research Institute in Kisumu. The insectary was not regulated for temperature and humidity; ambient temperature (average [approximately equal to] 24[degrees]C) and humidity ([approximately equal to] 75% relative humidity) were used for the study. Emerged adults were fed with 10% sucrose solution, and 2- to 5-day-old females were used to determine insecticide susceptibility by using the standard World Health Organization (WHO) insecticide susceptibility tube test http://www.who.int/ malaria/publications/atoz/9789241505154/en/. Four classes of insecticides were tested, including pyrethroids lambdacyhalothrin (diagnostic dose 0.05%), deltamethrin (4%), and permethrin (0.75%); organochlorine DDT (0.05%); organophosphate malathion (5%); and carbamate bendiocarb (0.1%) (11). The WHO-designated, pyrethroid-susceptible An. gambiae mosquito in Kisumu was used as a control.
Mosquitoes were exposed to each insecticide for 1 h and then maintained in holding tubes with 10% sucrose solution for 24 h. Mortality rates were scored after the 24-h recovery period; the susceptibility status of the mosquito populations was graded according to WHO criteria (11). Knockdown time (time required to render an adult mosquito unable to fly) was recorded every 10 minutes. Tests were done at 26[degrees]C [+ or -] 2[degrees]C and 80% [+ or -] 10% relative humidity during the 1-h exposure period and the subsequent 24-h period during which the mosquito would die or recover, with a 12D:12N photoperiod. We tested 200 mosquitoes per site per insecticide; that is, 8 replicates of exposure and 2 replicates of control, with 20 mosquitoes per replicate. A total of 8,400 (200 per site x 7 sites x 6 insecticides) female mosquitoes were tested. Knockdown rates are provided in the online Technical Appendix Figure (http://wwwnc.cdc. gov/EID/article/21/12/15-0814-Techapp1.pdf).
We identified species of a subset of randomly selected susceptible and resistant mosquitoes from the bioassay by using 16s rDNA PCR (12). A total of 1,002 specimens were molecularly identified. The real-time TaqMan assay was used to detect knockdown resistance (kdr) gene mutations and genotypes at amino acid position L1014 of the voltage-gated sodium channel gene (12). A total of 579 mosquitoes were examined for kdr mutation.
Results of WHO susceptibility bioassays showed a 100% mortality rate in the susceptible Kisumu An. gambiae reference strain after exposure to all insecticides tested and 50.4%-87.2% in the 7-field An. gambiae sensu lato populations resulting from exposure to all pyrethroids and DDT. These field populations were highly resistant to pyrethroids, demonstrated by an observed mortality rate that was considerably less than the WHO 90% threshold for resistance. The Bungoma population was the most resistant, exhibiting only a 50% mortality rate against permethrin. The WHO susceptibility bioassay also indicated that An. gambiae sensu lato was highly resistant to DDT: mortality rates ranged 50.4%-73.2% at all sites (Figure 2). Five of the 7 study populations were susceptible to bendiocarb, but 2 populations (Iguhu and Bungoma) were resistant (Figure 2). A 100% mortality rate was observed in mosquito populations exposed to malathion at all sites (Figure 2).
PCR analysis found that An. gambiae sensu stricto (s.s.) was the predominant species in Chulaimbo (72.0%), Iguhu (88.0%), Bungoma (90.0%), Emakakha (93.4%), and Emutete (94.0%), whereas An. arabiensis was predominant in Kisian (64.4%) and Ahero (89.3%) (Table 1). The L1014F mutation was not detected in An. gambiae s.s or An. arabiensis mosquitoes at any sites. Frequency of L1014S point mutation was high for An. gambiae s.s. (85.8%-92.9%) except in the Kisian population (33.0%) (Table 2). For An. arabiensis, L1014S mutation frequency was lower (1.2%-39.1%). Homozygosity of L1014S genotype was high in An. gambiae s.s (30.0%-89.3%), but low in An. arabiensis (0-39.1%) (Table 2).
We found through a survey that pyrethroids were the most frequently used insecticide for mosquito control (online Technical Appendix Table). Pyrethroids were also frequently used for control of livestock disease vectors and agricultural pests. Most (73.3%-96.6%) surveyed households used pyrethroids for malaria vector control in the form of ITNs and IRS (online Technical Appendix Table). Carbamate was mainly used for livestock disease vector control, and organophosphate was used seasonally for crop pest control among a small proportion of households.
This study found high resistance to pyrethroid insecticide in all 7 study populations, no resistance to organophosphate, and patchy distribution of resistance to carbamate insecticide in An. gambiae and An. arabiensis mosquitoes in western Kenya. This finding has critical implications in guiding malaria vector control in Kenya. In Kenya, current policy on IRS use of insecticides is limited to pyrethroids and DDT (13). Considering widespread pyrethroid resistance, non-pyrethroid-based vector control tools may be preferable. There is a growing debate among government decision makers on whether to use organophosphates (such as malathion or chlorpyrifos methyl) and carbamates (such as bendiocarb) for IRS in Kenya. Our finding on the complete susceptibility to organophosphates in malaria vectors suggests that organophosphates are a potentially effective insecticide for IRS. The patchy distribution of resistance to carbamates calls for careful resistance baseline monitoring if carbamates are considered for IRS.
Although we detected widespread and strong phenotypic resistance to pyrethroids in An. gambiae mosquitoes, whether this resistance could result in operational ITN or IRS malaria control failure in the field is unknown. A report from Cote d'Ivoire showed that ITNs remained effective in reducing entomological inoculation rate in an area of higher kdr frequency in An. gambiae mosquitoes (14). Similarly, a cohort study in Malawi found that the use of ITNs reduced the incidence of cases of malaria by 30% in children in an area that has documented moderate levels of pyrethroid resistance and considerable malaria transmission (15). Cost-effectiveness is another consideration. A thorough assessment of the effect of resistance to pyrethroids on the efficacy and cost-effectiveness of LLINs and IRS for malarial disease and transmission will clarify the need to consider a shift from pyrethroids to alternative carbamate or organophosphate insecticides or to other integrated strategies to control malaria.
DOI: http://dx.doi.org/ 10.3201/eid2112.150814
We thank the staff of the Climate and Human Health Research Unit, Centre for Global Health Research, Kenya Medical Research Institute, Kenya, for field assistance. We thank 2 anonymous reviewers for comments and suggestions that greatly improved the manuscript.
This paper was published with permission from the director of Kenya Medical Research Institute. This study was supported by grants from the National Institutes of Health (R01 A1050243 and D43 TW001505).
Ms. Wanjala is a PhD candidate at Kenyatta University and a trainee supported by a research training grant from the National Institutes of Health. Her research interests include vector ecology and malaria epidemiology.
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Christine L. Wanjala, Jernard P. Mbugi, Edna Ototo, Maxwell Gesuge, Yaw A. Afrane, Harrysone E. Atieli, Guofa Zhou, Andrew K. Githeko, Guiyun Yan
Author affiliations: Kenyatta University, Nairobi, Kenya (C.L. Wanjala, J.P. Mbugi, E. Ototo); Kenya Medical Research Institute, Kisumu, Kenya (C.L. Wanjala, E. Ototo, M. Gesuge, YA. Afrane, H.E. Atieli, A.K. Githeko); Masinde Muliro University of Science and Technology, Kakamega, Kenya (C.L. Wanjala); Program in Public Health, University of California, Irvine, USA (G. Zhou, G. Yan)
Address for correspondence: Guiyun Yan, Program in Public Health, University of California, Irvine, CA 92697, USA; email: email@example.com
Table 1. Anopheles mosquitoes observed for insecticide resistance in 7 study sites, Western Kenya, 2012-2013 Study site No. % An. % An. % Not collected arabiensis gambiae amplified subsp. Ahero 56 89.3 5.4 5.4 Kisian 225 64.4 32.9 2.4 Chulaimbo 100 24.0 72.0 4.0 Emutete 200 3.5 94.0 2.5 Emakakha 61 3.3 93.4 3.3 Iguhu 300 8.0 88.0 4.0 Bungoma 60 3.3 90.0 6.7 Table 2. Distribution of knockdown resistance genotypes and mutation frequencies by Anopheles mosquito species and study sites of pyrethroid-and DDT-resistant, organophosphate-susceptible Anopheles mosquitoes, Western Kenya, 2012-2013 * An. gambiae Study site No. LL LS SS Frequency, % Ahero ND ND ND ND ND Kisan 50 32 3 15 33.0 Chulaimbo 56 2 4 50 92.9 Emutete 87 7 4 76 89.7 Emakakha 57 1 7 49 92.1 Iguhu 108 10 7 91 87.5 Bungoma 53 5 5 43 85.8 An. arabiensis Study site No. LL LS SS Frequency, % Ahero 50 46 4 0 4.0 Kisan 42 41 1 0 1.2 Chulaimbo 23 14 0 9 39.1 Emutete ND ND ND ND ND Emakakha ND ND ND ND ND Iguhu 16 15 1 0 3.1 Bungoma ND ND ND ND ND * LL, wild genotype at L1014 codon; SS, homozygous genotype for L1014S mutation; LS, heterozygous genotype; Frequency, allele frequency of L1014S mutation. ND, not done because of insufficient number of specimens.
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|Author:||Wanjala, Christine L.; Mbugi, Jernard P.; Ototo, Edna; Gesuge, Maxwell; Afrane, Yaw A.; Atieli, Harr|
|Publication:||Emerging Infectious Diseases|
|Date:||Dec 1, 2015|
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