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Communication

Insecticide Exposure Triggers a Modulated Expression of ABC Transporter Genes in Larvae of Anopheles gambiae s.s.

by
Valentina Mastrantonio
1,†,
Marco Ferrari
2,3,†,
Agata Negri
1,2,
Tommaso Sturmo
1,
Guido Favia
4,
Daniele Porretta
1,
Sara Epis
2,* and
Sandra Urbanelli
1
1
Department of Environmental Biology, Sapienza University of Rome, 00185 Rome, Italy
2
Department of Biosciences and Pediatric Clinical Research Center, University of Milan, 20133 Milan, Italy
3
Texas Biomedical Research Institute, San Antonio, TX 78227, USA
4
School of Bioscience and Veterinary Medicine, University of Camerino, 62032 Macerata, Italy
*
Author to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Insects 2019, 10(3), 66; https://doi.org/10.3390/insects10030066
Submission received: 22 January 2019 / Revised: 21 February 2019 / Accepted: 28 February 2019 / Published: 5 March 2019
(This article belongs to the Special Issue Integrative Mosquito Biology: From Molecules to Ecosystems)
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Abstract

:
Insecticides remain a main tool for the control of arthropod vectors. The urgency to prevent the insurgence of insecticide resistance and the perspective to find new target sites, for the development of novel molecules, are fuelling the study of the molecular mechanisms involved in insect defence against xenobiotic compounds. In this study, we have investigated if ATP-binding cassette (ABC) transporters, a major component of the defensome machinery, are involved in defence against the insecticide permethrin, in susceptible larvae of the malaria vector Anopheles gambiae sensu stricto. Bioassays were performed with permethrin alone, or in combination with an ABC transporter inhibitor. Then we have investigated the expression profiles of five ABC transporter genes at different time points following permethrin exposure, to assess their expression patterns across time. The inhibition of ABC transporters increased the larval mortality by about 15-fold. Likewise, three genes were up-regulated after exposure to permethrin, showing different patterns of expression across the 48 h. Our results provide the first evidences of ABC transporters involvement in defence against a toxic in larvae of An. gambiae s.s. and show that the gene expression response is modulated across time, being continuous, but stronger at the earliest and latest times after exposure.

1. Introduction

Vector-borne diseases, caused by pathogens and parasites transmitted by bloodsucking arthropods, such as mosquitoes, sandflies, ticks, and tse-tse flies, are a major threat to human health and well-being [1]. Among them, malaria, transmitted by Anopheles mosquitoes, is undoubtedly one of the most serious life-threating diseases for humans [1]. Vector control through insecticides remains a main tool for malaria prevention, although progress toward the development of alternative or complementary vector control strategies has been made [2,3]. However, environmental pollution and the increasing insecticide resistance are seriously hampering the use of insecticides and their efficacy. Resistant mosquitoes, belonging to different species, have indeed been recorded in 64 countries with ongoing malaria transmission, with resistance to pyrethroids, being the most common [4,5,6].
Chemical detoxification is likely to play an important role in the development of insecticide resistance. Detoxification in insects is achieved through an array of protein systems, including detoxifying enzymes and efflux pump transporters [7,8,9,10,11]. Natural selection can act on the genes coding for detoxifying proteins, promoting the evolution of metabolic resistance. In susceptible strains, the assessment of the expression of detoxifying genes in response to insecticides could contribute to the comprehension of the molecular mechanisms underlying insecticide detoxification. Furthermore, detoxifying genes could be exploited as targets for novel classes of insecticide compounds. For example, the inhibition of detoxifying efflux pumps has been shown to increase the susceptibility to insecticides in several arthropod species, including malaria vectors [7,8,9,10]. Combined treatments of insecticides with inhibitors of efflux pump transporters could therefore allow to reduce the dose and frequency of insecticide applications and to generate a cascade of positive effects (e.g., reduction of the risk of resistance development, minor pesticide pollution and reduced damage to non-target fauna) [12,13]. In this context, a major goal is to identify the genes encoding for the detoxifying proteins in order to achieve species- and gene-specific inhibition [7,8,9,10].
ATP-binding cassette (ABC) transporters are ATP-dependent efflux pumps, located in the cellular membrane of prokaryotic and eukaryotic organisms, belonging to the ATP-binding cassette (ABC) transporter family. Among the eight sub-families (i.e., ABCB-ABCH) included in the ABC family, three of them, ABCB, ABCC and ABCG, are involved in xenobiotic detoxification. ABC transporters are part of a wider defence system comprising several gene families and pathways that allow an organism to transform and eliminate toxic chemicals (chemical defensome) [12,13,14,15,16,17,18,19].
In recent years, several studies have documented that ABC transporters play an important role in insecticide detoxification in a variety of arthropod species, ranging from ticks, to bed bugs, to body lice and mosquitoes [9,13,19,20,21,22,23,24,25]. On the other hand, the pattern of ABC transporter involvement in insecticide detoxification is different in different strains (resistant vs. susceptible), life-stages (adults vs. larvae) and sexes of the same species [8,26,27]. In addition, even though ABC transporters can act against all major insecticide classes, including organochlorines, organophosphates, pyrethroids and even Bacillus thuringensis (Bt) toxins, some heterogeneity can be observed within and between species [14,28]. For example in the mosquito Culex pipiens, ABC transporters have been shown to be involved against endosulfan, ivermectin and cypermethrin, but not against chlorpyrifos [24]. Likewise, ABC transporters were shown to be involved against temephos in the mosquitoes Aedes caspius [13] and Ae. aegypti [10], but not in Anopheles stephensi [15]. Further studies are thus required to determine the occurrence of common patterns in ABC transporter engagement, in relation with taxa or insecticide classes.
This study is focused on the mosquito Anopheles gambiae sensu stricto, the principal malaria vector in sub-Saharan African regions, and on the pyrethroid insecticide permethrin. Pyrethroids, among the different classes of insecticides recommended by the World Health Organization (WHO), still occupy a prominent position in malaria vector control. They are indeed widely used on approved long-lasting insecticidal nets (LLINs) and indoor residual spraying programmes (IRS) to control adult mosquitoes [1].
In the case of An. gambiae s.s., there are circumstantial evidences for the involvement of ABC transporters in pyrethroid resistance, i.e., the results from a whole genome-transcriptomic study, showing a constitutive over-expression of one ABCC member in adult deltamethrin-resistant individuals [29]. More recently, ABC transporters have been shown to be involved in the resistance against pyrethroids in adult individuals [20]. In addition, due to the wide use of pyrethroids in crop pest control, also larval stages of An. gambiae can be exposed to these insecticides in the developing sites near crop fields, which would lead to a further risk of insecticide resistance insurgence [30,31,32]. To date, however, no studies have been focused on the role of ABC transporters against pyrethroids in larval stages of this species. Here, we investigated the potential association between ABC transporters and permethrin using both laboratory bioassays and gene induction experiments. We conducted laboratory bioassays with permethrin alone or in combination with an ABC transporters inhibitor, to assess if these efflux pumps are a mechanism of defence against this insecticide in the larval stage. In the genome of An. gambiae, 34 ABC transporter genes have been identified [14]. Among them, we investigated the expression profiles of five genes encoding for ABC transporters that were previously found involved in insecticide detoxification in other arthropod species [10,33,34,35,36,37,38].

2. Materials and Methods

2.1. Mosquitoes

All mosquito larvae used in this study derived from an An. gambiae s.s. colony from the University of Camerino (Camerino, Italy), previously tested for its susceptibility to permethrin (2 < ratio RR50 < 5, according to Fossog and coworkers [39]). This colony was obtained in 2008 from the Centre National de Recherche et de Formation sur le Paludisme (CNRFP) in Ouagadougou (Burkina Faso, West Africa), and descended from wild mosquitoes collected in Burkina Faso. Mosquitoes have then been reared for about 9 years in the Camerino insectary, where they were maintained at standard lighting conditions of 12 h light and 12 h dark, a relative humidity of 80 ± 5% and temperature of 30 °C, in aseptic conditions during both the immature and adult stages. The larvae were grown in tanks filled with culture water containing sterile minced commercial mouse food.

2.2. Bioassays

In order to assess if ABC transporters are involved against permethrin in larvae of An. gambiae s.s., bioassays with insecticide, alone or in combination with a sub-lethal dose of the ABC inhibitor verapamil, were carried out, according to standard protocols [32]. Groups of 25 third-instar larvae were placed into 250 mL plastic cups with 100 mL of spring water, and then insecticide or insecticide plus inhibitor were added. In the bioassays with insecticide alone, six concentrations of permethrin (PESTANAL, Sigma-Aldrich S.r.l., Milan, Italy) were used, ranging from 15 to 700 ppb (i.e., 15, 47, 92, 230, 350 and 700 ppb), leading to a mortality from 1 to 99%. In the bioassays with insecticide and insecticide plus verapamil, four concentrations were tested: 4.8, 15, 47 and 92 ppb. To determinate the sub-lethal dose of verapamil (i.e., the highest dose at which no dead larvae were observed) six concentrations were used (20, 40, 80, 100, 160 and 240 ppm). Larvae treated only with acetone (the solvent of permethrin, Sigma-Aldrich S.r.l., Milan, Italy) and water were also included as controls. All experiments were performed in quadruplicate. Mortality data were registered at 24 h after treatment and analysed by Probit regression analysis to estimate LD50 dose and their 95% confidence intervals (CIs) using the Poloplus software [40].
The synergistic ratio was then calculated from the LD50 doses estimated from the treatments using permethrin and permethrin plus verapamil to assess the effect of the ABC transporters inhibition on the An. gambiae s.s. larvae. The hypotheses of equality (equal slopes and intercepts) and parallelism (equal slopes) of the regression lines of the two treatments were also tested using the likelihood-ratio test, as implemented in the software Poloplus.

2.3. Induction of ABC Transporter Gene Expression

Five genes encoding for ABC transporters were analyzed for their expression profiles in treated or untreated larvae of An. gambiae s.s: three members of the ABCB sub-family (i.e., AGAP005639, AGAP006273, AGAP002278); one member of the ABCC sub-family (AGAP006427); and one member of sub-family ABCG (AGAP001333). They were selected in order to investigate members of all ABC transporter sub-families involved in insecticide defence (ABCB, ABCC and ABCG), and on the basis of previous studies showing their involvement against insecticides in susceptible and resistant insect species [10,33,34,35,36,37,38].
Oligonucleotide primers were designed from the sequences of each gene using the Primer3, Beacon DesignerTM and mFold softwares [41] and used for standard and quantitative RT-PCRs. In order to confirm the specificity of the amplifications, the amplicons obtained using standard PCR conditions (see below) were sequenced and the obtained sequences blasted into the Genbank database.
In order to analyze the expression profile of ABC transporter genes after permethrin exposure, mosquito larvae were treated with the insecticide following the protocol described above. The LD50 dose of permethrin (297.84 ppb), estimated by the above bioassays, was used to treat the larvae; larvae at five time-points after exposure (2, 4, 6, 24 and 48 h) were collected and analyzed. Six replicas were effected for each time point. Three pools of 10 individuals, each pool from two plastic vessels, were collected at the five time-points, and stored in RNA later at −80 °C until subsequent molecular analysis. Negative controls (larvae treated only with acetone and water), were also collected for each time of exposure. RNA was extracted from each pool of individuals using the RNeasy Mini Kit (Qiagen, Hilden, Germany), according to the manufacturer’s instructions. Then, total RNA was eluted into nuclease-free water and the concentration of RNA was determined at 260 nm using a NanoDrop ND-2000 (Thermo Fisher Scientific, Waltham, MA, USA). cDNAs were synthesized from 150 ng of total RNA using a QuantiTect Reverse Transcription Kit (Qiagen, Hilden, Germany) with random hexamers. The cDNA was used as template in reverse transcription (RT)-PCR reactions using the primers reported in Table 1.
RT-PCRs on target genes were performed using a BioRad CFX Real-Time PCR Detection System (Bio-Rad, Hercules, CA, USA) with the following conditions: 50 ng of cDNA; 250 nM of forward and reverse primers; 98 °C for 30 s, 40 cycles of 98 °C for 15 sec, 57–59 °C for 30 sec; fluorescence acquisition at the end of each cycle; melting curve analysis after the last cycle. In order to analyze the expression of the target genes, the efficiency of the new primer pairs was assessed trough the analysis of the standard curves, then the cycle threshold (Ct) values were determined for each gene and normalized according to two endogenous reference genes: the ribosomal protein S7 (rps7) gene and the actin gene (act 5C) (Table 1). The expression of ABC transporters genes in the control group was considered as the basal level. Shapiro–Wilk test was performed to check normality of the normalized expression data. For each gene, univariate two-way ANOVA was performed to compare differences in relative expression between treated and control larvae and among time points. Subsequent post-hoc Tukey tests were performed for pairwise comparisons among time points. All analyses were performed using the software IBM SPSS Statistics (IBM Corp. Released 2013, Armonk, NY, USA).

3. Results

3.1. Laboratory Bioassays

The sub-lethal dose of the inhibitor verapamil was 80 ppm, as no mortality was observed at this concentration, while dead larvae were observed from the 100 ppm concentration (Figure S1). Mortality data of the bioassays with insecticide and insecticide plus verapamil recorded at 24 h were well described by the probit dose–response model (chi-squared goodness-of-fit test, p > 0.05). Both the hypotheses of the regression line equality and parallelism between treatments were rejected, showing significant differences between the two treatments (Table 2).
The LD50 dose and 95% Confidence Intervals (CIs) estimated was 297.84 ppb (248.5–368.18) for the treatment with permethrin alone, and 18.69 ppb (15.89–21.81) for treatment with insecticide plus verapamil. A synergistic factor of 15.94 (12.37–20.53) was estimated between the LD50 of the two treatments (Table 2, near here).

3.2. Expression Profiles of ABC Transporter Genes after Permethrin Exposure

The sequencing of the amplicons obtained by conventional PCRs confirmed the specificity of the amplification for each selected ABC transporter gene, with an identity of 100% with the sequences of the ABC transporter genes of An. gambiae s.s. available in the databases.
All primer pairs used to amplify ABC transporter genes showed an efficiency ranging from 95% to 105%. The results obtained from gene expression analyses for each gene in treated larvae, in comparison with the untreated larvae, are shown in Figure 1 and Table S1.
The Shapiro–Wilk test showed normal distribution of the data (all tests p > 0.05). The ANOVA analysis showed that the expression levels of all ABC genes analysed were significantly affected by permethrin treatment, by the time of larval exposure and by the combination of these two factors (Table S2). For each gene, post-hoc Tukey tests showed significant differences among the expression levels across time (Figure 1).

4. Discussion

4.1. Involvement of ABC Transporters in Permethrin Detoxification

The use of ABC transporter inhibitors has greatly contributed to document the involvement of these efflux pumps in defence/resistance against insecticides in arthropod vectors [14]. More recently, transcriptional studies allowed not only to further support the detoxifying role of ABC transporters, but also to identify which genes encoding for ABC transporters are mainly involved [12,14,15]. In this study, using both of the above experimental approaches, we have provided evidence for the involvement of ABC transporters in the defence against permethrin in larvae of An. gambiae s.s. By exposing third-instar larvae to the LD50 dose of permethrin, indeed, we observed that mortality was about 15-fold greater after the treatment with insecticide plus ABC inhibitor, than after treatment with insecticide alone (Table 2). Likewise, the exposure of larvae to the insecticide led to transcriptional induction of three out of the five ABC transporter genes analyzed (Figure 1), which further supports the involvement of ABC transporters in the defence against permethrin [14].
Among the ABC transporter genes analyzed in An. gambiae s.s., some of them showed an activation pattern similar to that observed in other insect species. For example, genes orthologues to the ABCG-AGAP001333 gene here examined have been shown to be over-transcribed in Anopheles arabiensis and in An. stephensi mosquitoes exposed to Dichlorodiphenyltrichloroethane (DDT) and permethrin, respectively [19,33,34,35]. These results indicate that this ABCG transporter is likely to play an important role in different mosquito species (as well as in other insects, e.g., in Bemisia tabaci exposed to neonicotenoids [38]) as a defence system against different insecticides. Notably, the AnstABCG4 transporter gene (ASTE008861) of An. stephensi was found over-expressed after 2, 4, 6, 24 and 48 h of exposure to the LD50 dose of permethrin [34], which is the same pattern that we observed in An. gambiae s.s. larvae. The comparison of the expression profiles in An. gambiae s.s. and An. stephensi susceptible larvae, exposed to LD50 permethrin dose, not only suggests that the ABCG4 transporter is involved in defence against permethrin in both species, but also shows that the induction pattern is similar. Similarity between the two species can also be observed in the transcriptional response of the orthologous genes ABCB-AGAP006273 and ASTE000608/AnstABCB3: in the larvae of both species, no-differential expression or up-regulation were observed during the 2–48 h of permethrin exposure.
The other ABC transporters analysed in An. gambiae s.s. showed a more heterogeneous involvement among species and insecticides. This is the case of the ABCB-AGAP002278 gene that showed no transcriptional induction by permethrin in An. gambiae s.s. larvae (Figure 1), while its orthologous in An. stephensi (ASTE003466/AnstABCBmember6) was found up-regulated in larvae exposed to this insecticide [33,34]. Similarly, the ABCB-AGAP005639 gene, that we found up-regulated in An. gambiae s.s. after 4 and 48 h of exposure, was found down-regulated in previous studies on An. stephensi (ASTE009548/AnstABCB2) [33,34]. Interestingly, in susceptible larvae of the mosquito Aedes aegypti, the transporter AaegP-gp–AAEL010379-PA, orthologous to the An. gambiae s.s. ABCB-AGAP005639, showed an increased expression of about eight-fold compared to control after 48 h of exposure to the LD50 dose of the organophosphate temephos, which supports its involvement in temephos defence [10]. In summary, although some similarities exist between species in the response to insecticides, more studies are needed to assess if there are conserved patterns.
Regarding An. gambiae s.s, future studies addressing the gene expression of other ABC transporter genes during insecticide exposure are needed to gain a more comprehensive picture of how many ABC transporter genes are involved in the defense against permethrin. Furthermore, mRNA expression studies could also be addressed to analyse the ABC transporter gene expression, not only after the exposure to the toxic, but also after treatment with ABC transporter inhibitors or after treatment with inhibitors in combination with insecticides. For example, the exposure to verapamil of MCF-7 human mammary carcinoma cell lines and hepatocellular carcinoma has been shown to reduce the expression levels the MDR1 ABC transporter gene [42,43]. Likewise, a significant decrease in P-gp expression and transport activity has been observed when L1210/VCR neoplastic cells were treated with transretinoic acid (ATRA) and verapamil [44]. Although the mechanism of down-regulation of ABC transporter genes by verapamil is not known, these data suggest that it might influence the ABC transporters at both protein and mRNA levels. In arthropods, at our best knowledge, verapamil has been used only as synergist and no data are available about the expression levels of ABC transporter genes under verapamil exposure, alone or in combination with an insecticide [14]. If a down-regulation effect of ABC transporter genes by verapamil would exist, as in human cancer cell lines, it could in part explain the lethal effect on exposed larvae to permethrin plus verapamil. Furthermore, the analyses of the expression patterns in larvae exposed to verapamil or in association with permethrin could contribute to describe the possible involvement of ABC transporter genes in cellular defense.

4.2. Dynamics of Gene Transcriptional Induction during Permethrin Exposure

The dynamics of the detoxifying gene activation during insecticide exposure is currently poorly investigated in arthropods [19,27,33,34]. Most of the studies that analysed the transcriptional response of defensome genes [19] after insecticide exposure have indeed been focused on a single time point [14]. Some studies that have recently investigated the expression profiles of detoxifying genes at different time points during insecticide exposure, are showing that defence response to insecticide stress is a dynamic process where the genes involved in the cellular defence can turn on and off at different time points during insecticide exposure [19,34,45,46,47,48].
With respect to the ABC transporters, this pattern can be due to the specificity between insecticide substrate and the transporter. Different ABC transporter genes have been indeed shown to be up regulated against different insecticides within the same species [8,15,26,27]. Furthermore, the high cost of detoxification can led to a reallocation of the energetic resources and, consequently, to the turn off of some genes during insecticide exposure. Two out the five ABC transporter genes analysed in An. gambiae s.s. were down-regulated or not significantly up-regulated during the permethrin exposure, which supports the above view (Figure 1).
The analysis of gene expression profiles across time allowed us to show not only which genes encoding for ABC transporters were up-regulated, but also the dynamics of their transcriptional response during permethrin exposure. The three genes that were found up-regulated in An. gambiae s.s., showed different patterns of expression across the 48 h of permethrin exposure. The ABCB-AGAP005639 was found up-regulated only at 4 and 48 h with a peak of expression registered at 48 h post-exposure (i.e., about eight-fold compared to control). The ABCG-AGAP001333 gene was up-regulated since 2 hours after treatment and its up-regulation persisted until 48 h maintaining similar values across time, similarly to the ABCC-AGAP006427 gene (with the exception of 24 h) (Figure 1). These results showed therefore the occurrence of a modulated response of the ABC transporter genes across time, where each single gene is up- or down-regulated during insecticide exposure at different time-points, and up-regulation of multiple genes occurs at different time-points. By considering the profiles of all up-regulated genes during permethrin exposure, a more general expression pattern can be observed that is consistent with the role of ABC transporters in the Phases 0 and III during the detoxification process [17,18,19]. Consistently, it can be observed that some genes were up-regulated across all time points from 6 to 48 h (ABCC-AGAP006427 and ABCG-AGAP001333) as well as that the ABCB-AGAP005639 gene was up-regulated at early or late time-points (e.g., 4 and 48 h), which depicts a continuous action of ABC transporters across time and would suggest a stronger response at the earliest and latest times after exposure as observed also in the An. stephensi mosquito [19].

5. Conclusions

The urgency to protect the current chemical weapons used to control arthropod vectors from resistance insurgence and the perspective to find new target sites are fuelling the study of the molecular defence mechanisms against insecticides. In this study, we provide evidences for the involvement of ABC transporter efflux pumps in defence against permethrin in An. gambiae s.s. larvae. By analysing the expression profiles of ABC transporter genes at several time points, moreover, we found three genes up-regulated throughout the time of permethrin exposure (48 h). Although exposure time and insecticide dose can affect gene induction, as well as only a subset of the ABC transporter genes has been analysed, our results clearly support the occurrence of a modulated transcriptional response during insecticide exposure in An. gambiae s.s. This is consistent with the patterns observed for ABC transporters in the mosquito An. stephensi [19,33,34], or in other gene families involved in xenobiotic defence, such as CYP450 [45,46] and Cuticular Proteins (CPs) [48]. Future studies should be directed toward the analysis of induction of all defensome genes to understand how they work together during insecticide stress and to find key genes that could be potential targets for the development of gene-silencing based control tools.

Supplementary Materials

The following are available online at https://www.mdpi.com/2075-4450/10/3/66/s1, Figure S1: Mortality rate of Anopheles gambiae s.s. larvae treated with verapamil, Table S1: Relative expression of Anopheles gambiae s.s. ABC genes measured by quantitative PCR after permethrin exposure at different times, Table S2: Univariate two-way ANOVA analysis on relative gene expression in relation to insecticide treatment and time of exposure for each ABC transporter gene analysed.

Author Contributions

Conceptualization, V.M., D.P. and S.E.; Methodology, V.M. and D.P.; Formal Analysis V.M., M.F., T.S. and A.N.; Resources, S.E. and G.F.; Writing—Original Draft Preparation, M.F., V.M., S.U. and S.E.

Funding

This study was supported by the MIUR (Italian Minister of University and Research) and by the Progetto Ateneo (Bando Ricerca Uniroma1, RM116154C9CFDE3B).

Acknowledgments

We would like to thank the Editor and three anonymous reviewers for their comments, Veronica Rovazzani and Giulia Scuccimarra for their help in experiments, Mark Eltenton for the linguistic revision.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. WHO. Eliminating Malaria; World Health Organization: Geneva, Switzerland, 2016. [Google Scholar]
  2. McGraw, E.A.; O’Neill, S.L. Beyond insecticides: New thinking on an ancient problem. Nat. Rev. Microbiol. 2013, 11, 181–193. [Google Scholar] [CrossRef] [PubMed]
  3. Wilke, A.B.; Marrelli, M.T. Paratransgenesis: A promising new strategy for mosquito vector control. Parasit. Vectors 2015, 8, 342. [Google Scholar] [CrossRef] [PubMed]
  4. WHO. Global Plan for Insecticide Resistance Management; World Health Organization: Geneva, Switzerland, 2012; p. 130. [Google Scholar]
  5. Liu, N. Insecticide resistance in mosquitoes: Impact, mechanisms and research directions. Annu. Rev. Entomol. 2015, 60, 537–559. [Google Scholar] [CrossRef] [PubMed]
  6. Ranson, H.; Lissenden, N. Insecticide Resistance in African Anopheles Mosquitoes: A Worsening Situation that Needs Urgent Action to Maintain Malaria Control. Trends Parasitol. 2016, 32, 187–196. [Google Scholar] [CrossRef] [PubMed]
  7. Chouaïbou, M.; Zivanovic, G.B.; Knox, T.B.; Jamet, H.P.; Bonfoh, B. Synergist bioassays: A simple method for initial metabolic resistance investigation of field Anopheles gambiae s.l. populations. Acta Trop. 2014, 130, 108–111. [Google Scholar] [CrossRef] [PubMed]
  8. Pohl, P.C.; Klafke, G.M.; Carvalho, D.D.; Martins, J.R.; Daffre, S.; da Silva Vaz, I. Jr.; Masuda, A. ABC transporter efflux pumps: A defence mechanism against ivermectin in Rhipicephalus (Boophilus) microplus. Int. J. Parasitol. 2011, 41, 1323–1333. [Google Scholar] [CrossRef] [PubMed]
  9. Yoon, K.S.; Strycharz, J.P.; Baek, J.H.; Sun, W.; Kim, J.H.; Kang, J.S.; Pittendringh, B.R.; Lee, S.H.; Clarck, J.M. Brief exposures of human body lice to sublethal amounts of ivermectin over-transcribes detoxification genes involved in tolerance. Insect Mol. Biol. 2011, 20, 687–699. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  10. Figueira-Mansur, J.; Ferreira-Pereira, A.; Mansur, J.F.; Franco, T.A.; Alvarenga, E.S.; Sorgine, M.H.; Neves, B.C.; Melo, A.C.; Leal, W.S.; Masuda, H.; et al. Silencing of P-glycoprotein increases mortality in temephos-treated Aedes aegypti larvae. Insect Mol. Biol. 2013, 226, 648–658. [Google Scholar] [CrossRef] [PubMed]
  11. Bona, A.C.; Chitolina, R.F.; Fermino, M.L.; de Castro Poncio, L.; Weiss, A.; Lima, J.B.; Paldi, N.; Bernardes, E.S.; Henen, J.; Maori, E. Larval application of sodium channel homologous dsRNA restores pyrethroid insecticide susceptibility in a resistant adult mosquito population. Parasit. Vectors 2016, 14, 397. [Google Scholar] [CrossRef] [PubMed]
  12. Buss, D.S.; Callaghan, A. Interaction of pesticides with p-glycoprotein and other ABC proteins: A survey of the possible importance to insecticide: Herbicide and fungicide resistance. Pestic. Biochem. Physiol. 2008, 90, 141–153. [Google Scholar] [CrossRef]
  13. Porretta, D.; Gargani, M.; Bellini, R.; Medici, A.; Punelli, F.; Urbanelli, S. Defence mechanism against insecticides temephos and diflubenzuron in the mosquito Aedes caspius: The P-glycoprotein efflux pumps. Med. Vet. Entomol. 2008, 22, 48–54. [Google Scholar] [CrossRef] [PubMed]
  14. Dermauw, W.; van Leeuwen, T. The ABC gene family in arthropods: Comparative genomics and role in insecticide transport and resistance. Insect. Biochem. Mol. Biol. 2014, 45, 89–110. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Porretta, D.; Epis, S.; Mastrantonio, V.; Ferrari, M.; Bellini, R.; Favia, G.; Urbanelli, S. How heterogeneous is the involvement of ABC transporters against insecticides? Acta Trop. 2016, 157, 131–135. [Google Scholar] [CrossRef] [PubMed]
  16. Goldstone, J.; Hamdoun, A.M.; Cole, B.; Ashby, M.H.; Scally, M.; Dean, M.; Epel, D.; Hahn, M.E.; Stegeman, J.J. The chemical defensome: Environmental sensing and response genes in the Strongylocentrotus purpuratus genome. Dev. Biol. 2006, 300, 366–384. [Google Scholar] [CrossRef] [PubMed]
  17. Goldstone, J. Environmental Sensing and Response Genes in Cnidaria: The Chemical Defensome in the Sea Anemone Nematostella vectensis. Cell. Biol. Toxicol. 2008, 24, 483–502. [Google Scholar] [CrossRef] [PubMed]
  18. Steinberg, C.E.W. Arms Race between Plants and Animals: Biotransformation System. In Stress Ecology: Environmental Stress as Ecological Driving Force and Key Player in Evolution; Steinberg, C.E.W., Ed.; Springer: Dordrecht, The Netherlands, 2012; pp. 61–105. [Google Scholar] [CrossRef]
  19. De Marco, L.; Sassera, D.; Epis, S.; Mastrantonio, V.; Ferrari, M.; Ricci, I.; Comandatore, F.; Bandi, C.; Porretta, D.; Urbanelli, S. The choreography of the chemical defensome response to insecticide stress: Insights into the Anopheles stephensi transcriptome using RNA-Seq. Scien. Rep. 2017, 7, 41312. [Google Scholar] [CrossRef] [PubMed]
  20. Pignatelli, P.; Ingham, V.A.; Balabanidou, V.; Vontas, J.; Lycett, G.; Ranson, H. The Anopheles gambiae ATP-binding cassette transporter family: Phylogenetic analysis and tissue localization provide clues on function and role in insecticide resistance. Insect Mol. Biol. 2018, 27, 110–122. [Google Scholar] [CrossRef] [PubMed]
  21. Pohl, P.C.; Klafke, G.M.; Júnior, J.R.; Martins, J.R.; da Silva Vaz, I., Jr.; Masuda, A. ABC transporters as a multidrug detoxification mechanism in Rhipicephalus (Boophilus) microplus. Paras. Res. 2012, 111, 2345–2351. [Google Scholar] [CrossRef] [PubMed]
  22. Cafarchia, C.; Porretta, D.; Mastrantonio, V.; Epis, S.; Sassera, D.; Iatta, R.; Immediato, D.; Ramos, R.A.; Lia, R.P.; Dantas-Torres, F.; et al. Potential role of ATP-binding cassette transporters against acaricides in the brown dog tick Rhipicephalus sanguineus sensu lato. Med. Vet. Entomol. 2015, 29, 88–93. [Google Scholar] [CrossRef] [PubMed]
  23. Zhu, F.; Gujar, H.; Gordon, J.R.; Haynes, K.F.; Potter, M.F.; Palli, S.R. Bed bugs evolved unique adaptive strategy to resist pyrethroid insecticides. Sci. Rep. 2013, 3, 1456. [Google Scholar] [CrossRef] [PubMed]
  24. Buss, D.S.; McCaffery, A.R.; Callaghan, A. Evidence for p-glycoprotein modification of insecticide toxicity in mosquitoes of the Culex pipiens complex. Med. Vet. Entomol. 2002, 16, 218–222. [Google Scholar] [CrossRef] [PubMed]
  25. Lima, E.P.; Goulart, M.O.F.; Neto, M.L.R. Evaluation of the role of ATP-binding cassette transporters as a defence mechanism against temephos in populations of Aedes aegypti. Mem. Inst. Oswaldo Cruz 2014, 109, 964–966. [Google Scholar] [CrossRef] [PubMed]
  26. Valenzuela-Muñoz, V.; Nuñez-Acuña, G.; Gallardo-Escárate, C. Molecular characterization and transcription analysis of P-glycoprotein gene from the salmon louse Caligus rogercresseyi. J. Aquacult. Res. Dev. 2014, 5, 4. [Google Scholar] [CrossRef]
  27. Mastrantonio, V.; Ferrari, M.; Epis, S.; Negri, A.; Scuccimarra, G.; Montagna, M.; Favia, G.; Porretta, D.; Urbanelli, S.; Bandi, C. Gene expression modulation of ABC transporter genes in response to permethrin in adults of the mosquito malaria vector Anopheles stephensi. Acta Trop. 2017, 171, 37–43. [Google Scholar] [CrossRef] [PubMed]
  28. Heckel, D.G. Learning the ABCs of Bt: ABC transporters and insect resistance to Bacillus thuringiensis provide clues to a crucial step in toxin mode of action. Pestic. Biochem. Physiol. 2012, 104, 103–110. [Google Scholar] [CrossRef]
  29. Bonizzoni, M.; Afrane, Y.; Dunn, W.A.; Atieli, F.K.; Zhou, G.; Zhong, D. Comparative transcriptome analyses of deltamethrin-resistant and -susceptible Anopheles gambiae mosquitoes from Kenya by RNA-Seq. PLoS ONE 2012, 7, e44607. [Google Scholar] [CrossRef] [PubMed]
  30. Yadouleton, A.; Martin, T.; Padonou, G.; Chandre, F.; Asidi, A.; Djogbenou, L.; Dabiré, R.; Aïkpon, R.; Boko, M.; Glitho, I.; et al. Cotton pest management practices and the selection of pyrethroid resistance in Anopheles gambiae population in Northern Benin. Parasit. Vectors 2011, 4, 60. [Google Scholar] [CrossRef] [PubMed]
  31. Bigoga, J.D.; Ndangoh, D.N.; Ambene, P.H.A.; Patchoké, S.; Fondjo, E.; Leke, R.G. Pyrethroid resistance in Anopheles gambiae from the rubber cultivated area of Niete, South Region of Cameroon. Acta Trop. 2012, 124, 210–214. [Google Scholar] [CrossRef] [PubMed]
  32. Gnankiné, O.; Bassolé, I.H.N.; Chandre, F.; Glitho, I.; Akogbeto, M.; Dabiré, R.; Martin, T. Insecticide resistance in Bemisia tabaci Gennadius (Homoptera: Aleyrodidae) and Anopheles gambiae Giles (Diptera: Culicidae) could compromise the sustainability of malaria vector control strategies in West Africa. Acta Trop. 2013, 128, 7–17. [Google Scholar] [CrossRef] [PubMed]
  33. Epis, S.; Porretta, D.; Mastrantonio, V.; Urbanelli, S.; Sassera, D.; Rossi, P. ABC transporters are involved in defense against permethrin insecticide in the malaria vector Anopheles stephensi. Parasit. Vectors 2014, 7, 349. [Google Scholar] [CrossRef] [PubMed]
  34. Epis, S.; Porretta, D.; Mastrantonio, V.; Comandatore, F.; Sassera, D.; de Marco, L. Temporal dynamics of the ABC transporter response to insecticide treatment: Insights from the malaria vector Anopheles stephensi. Sci. Rep. 2014, 4, 7435. [Google Scholar] [CrossRef] [PubMed]
  35. Jones, C.M.; Toé, H.K.; Sanou, A.; Namountougou, M.; Hughes, A.; Diabaté, A.; Dabiré, R.; Simard, F.; Ranson, H. Additional selection for insecticide resistance in urban malaria vectors: DDT resistance in Anopheles arabiensis from Bobo-Dioulasso, Burkina Faso. PLoS ONE 2012, 7, e45995. [Google Scholar] [CrossRef] [PubMed]
  36. Merzendorfer, H. ABC Transporters and their role in protecting insects from pesticides and their metabolites. In Advances in Insect Physiology. Target Receptors in the Control of the Insect Pests: Part II; Cohen, E., Ed.; Academic Press: London, UK, 2014; pp. 1–73. [Google Scholar] [CrossRef]
  37. Tribble, N.D.; Burka, J.F.; Kibenge, F.S.B. Evidence for changes in the transcription levels of two putative P-glycoprotein genes in sea lice (Lepeophtheirus salmonis) in response to emamectin benzoate exposure. Mol. Biochem. Parasitol. 2007, 153, 59–65. [Google Scholar] [CrossRef] [PubMed]
  38. Yang, N.; Xie, W.; Yang, X.; Wang, S.; Wu, Q.; Li, R.; Pan, H.; Liu, B.; Shi, X.; Fang, Y.; et al. Transcriptomic and proteomic responses of sweetpotato whitefly, Bemisia tabaci, to thiamethoxam. PLoS ONE 2013, 8, e61820. [Google Scholar] [CrossRef] [PubMed]
  39. Fossog, T.B.; Kopya, E.; Ndo, C.; Menze-Djantio, B.; Costantini, C.; Njiokou, F.; Awono-Ambene, P.; Nkondjio, A.C. Water quality and Anopheles gambiae larval tolerance to pyrethroids in the cities of Douala and Yaoundé (Cameroon). J. Trop. Med. 2012, 429817. [Google Scholar] [CrossRef]
  40. Robertson, J.A.; Preisler, H.K.; Russell, R.M. Polo Plus: Probit and Logit Analysis; LeOra Software: Petaluma, CA, USA, 2003. [Google Scholar]
  41. Thornton, B.; Basu, C. Real-time PCR (qPCR) primer design using free online software. Biochem. Mol. Biol. Educ. 2011, 39, 145–154. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Dönmez, Y.; Akhmetova, L.; İşeri, Ö.D.; Kars, M.D.; Gündüz, U. Effect of MDR modulators verapamil and promethazine on gene expression levels of MDR1 and MRP1 in doxorubicin-resistant MCF-7 cells. Cancer Chemother. Pharmacol. 2011, 67, 823–828. [Google Scholar] [CrossRef] [PubMed]
  43. Jalali, A.; Ghasemian, S.; Najafzadeh, H.; Galehdari, H.; Seifi, M.R.; Zangene, F.; Dehdardargahi, S. Verapamil and rifampin effect on p-glycoprotein expression in hepatocellular carcinoma. J. Nat. Pharm. Prod. 2014, 10, e17741. [Google Scholar] [CrossRef]
  44. Sulová, Z.; Macejová, D.; Seres, M.; Sedlák, J.; Brtko, J.; Breier, A. Combined treatment of P-gp-positive L1210/VCR cells by verapamil and all-trans retinoic acid induces down-regulation of P-glycoprotein expression and transport activity. Toxicol. In Vitro 2008, 22, 96–105. [Google Scholar] [CrossRef] [PubMed]
  45. Liu, N.; Li, T.; Reid, W.R.; Yang, T.; Zhang, L. Multiple cytochrome P450 genes: Their constitutive overexpression and permethrin induction in insecticide resistant mosquitoes, Culex quinquefasciatus. PLoS ONE 2011, 6, e23403. [Google Scholar] [CrossRef] [PubMed]
  46. Gong, Y.; Li, T.; Zhang, L.; Gao, X.; Liu, N. Permethrin induction of multiple cytochrome P450 genes in insecticide-resistant mosquitoes, Culex quinquefasciatus. Int. J. Biol. Sci. 2013, 9, 863–871. [Google Scholar] [CrossRef] [PubMed]
  47. Doganlar, O.; Doganlar, Z.B. Responses of antioxidant enzymes and heat shock proteins in Drosophila to treatment with a pesticide mixture. Arch. Biol. Sci. Belgrade 2015, 67, 869–876. [Google Scholar] [CrossRef]
  48. Fang, F.; Wang, W.; Zhang, D.; Lv, Y.; Zhou, D.; Ma, L.; Shen, B.; Sun, Y.; Zhu, C. The cuticle proteins: A putative role for deltamethrin resistance in Culex pipiens pallens. Parasitol. Res. 2015, 114, 4421–4429. [Google Scholar] [CrossRef] [PubMed]
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Figure 1. Relative expression of Anopheles gambiae s.s. ABC genes measured by quantitative PCR after different times of permethrin exposure. The expression level in non-treated larvae was considered to be the basal level. The internal reference genes rps7 and act5C for An. gambiae s.s. were used to normalize the expression levels. The values are expressed as means ± standard deviations. In x-axes: time of permethrin exposure: 2, 4, 6, 24 and 48 h. For each gene, equal letter means post-hoc Tukey tests p > 0.05; different letter means post-hoc Tukey tests p < 0.05.
Figure 1. Relative expression of Anopheles gambiae s.s. ABC genes measured by quantitative PCR after different times of permethrin exposure. The expression level in non-treated larvae was considered to be the basal level. The internal reference genes rps7 and act5C for An. gambiae s.s. were used to normalize the expression levels. The values are expressed as means ± standard deviations. In x-axes: time of permethrin exposure: 2, 4, 6, 24 and 48 h. For each gene, equal letter means post-hoc Tukey tests p > 0.05; different letter means post-hoc Tukey tests p < 0.05.
Insects 10 00066 g001
Table
Table 1. Primer sequences used to amplify fragments of ATP-binding cassette (ABC) transporters genes in Anopheles gambiae s.s.
Table 1. Primer sequences used to amplify fragments of ATP-binding cassette (ABC) transporters genes in Anopheles gambiae s.s.
Vector Base Sequence IDABC Sub-FamilyForward 3’-5’Reverse 3’-5’PCR Product Size (bp)
AGAP005639ABCBTTCATCACGAAACTACCGAACGTCCCTTACTTGCTCGCT204
AGAP006273ABCBCACGCTGGGCTATCAGTAAAAACTTCCACCAATCGAAACG118
AGAP002278ABCBAAAGGTGACAGAGAGGTGTAGGAAAACGCCATGCACTAAACTATCACATT104
AGAP006427ABCCAAAGTGTTCTACGGCATGGTGAAGCAGCCTCCTTAATCGGTTTCAGTTT108
AGAP001333ABCGGTCTCCTGTCGTTGTAGTTTTCGTAACAGAAACATCGTCCATT174
AGAP010592rps7GGCGATCATCATCTACGTGCGTAGCTGCTGCAAACTTCGG459
AGAP000651act 5CTCTGGCACCACACGTTCTACCAGGTAGTCGGTGAGATCGC313
Table
Table 2. Toxicity of insecticide and insecticide + ABC transporters inhibitor. LD50, 95% Confidence Intervals (95% CI) and slopes estimated from mortality data by probit analysis are shown. SR, synergistic ratio.
Table 2. Toxicity of insecticide and insecticide + ABC transporters inhibitor. LD50, 95% Confidence Intervals (95% CI) and slopes estimated from mortality data by probit analysis are shown. SR, synergistic ratio.
InsecticideSlope (±SE)LD50 (95% CI)SR (95% CI)χ2 (df)
Goodness-of-FitEqualityParallelism
permethrin1.514 (0.131)297.84 ppb
(248.5–368.18)		 2.467 (4)317 (2) *11.40 (1) *
permethrin + verapamil2.259 (0.181)18.69 ppb
(15.89–21.81)		15.94
(12.37–20.53)		13.37 (5)
* Chi-Square probability p < 0.05.

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Mastrantonio, V.; Ferrari, M.; Negri, A.; Sturmo, T.; Favia, G.; Porretta, D.; Epis, S.; Urbanelli, S. Insecticide Exposure Triggers a Modulated Expression of ABC Transporter Genes in Larvae of Anopheles gambiae s.s. Insects 2019, 10, 66. https://doi.org/10.3390/insects10030066

AMA Style

Mastrantonio V, Ferrari M, Negri A, Sturmo T, Favia G, Porretta D, Epis S, Urbanelli S. Insecticide Exposure Triggers a Modulated Expression of ABC Transporter Genes in Larvae of Anopheles gambiae s.s. Insects. 2019; 10(3):66. https://doi.org/10.3390/insects10030066

Chicago/Turabian Style

Mastrantonio, Valentina, Marco Ferrari, Agata Negri, Tommaso Sturmo, Guido Favia, Daniele Porretta, Sara Epis, and Sandra Urbanelli. 2019. "Insecticide Exposure Triggers a Modulated Expression of ABC Transporter Genes in Larvae of Anopheles gambiae s.s." Insects 10, no. 3: 66. https://doi.org/10.3390/insects10030066

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