- Open Access
Yeast interfering RNA larvicides targeting neural genes induce high rates of Anopheles larval mortality
Malaria Journal volume 16, Article number: 461 (2017)
Although larviciding can reduce the number of outdoor biting malaria vector mosquitoes, which may help to prevent residual malaria transmission, the current larvicide repertoire is faced with great challenges to sustainability. The identification of new effective, economical, and biorational larvicides could facilitate maintenance and expansion of the practice of larviciding in integrated malaria vector mosquito control programmes. Interfering RNA molecules represent a novel class of larvicides with untapped potential for sustainable mosquito control. This investigation tested the hypothesis that short interfering RNA molecules can be used as mosquito larvicides.
A small interfering RNA (siRNA) screen for larval lethal genes identified siRNAs corresponding to the Anopheles gambiae suppressor of actin (Sac1), leukocyte receptor complex member (lrc), and offtrack (otk) genes. Saccharomyces cerevisiae (baker’s yeast) was engineered to produce short hairpin RNAs (shRNAs) for silencing of these genes. Feeding larvae with the engineered yeasts resulted in silenced target gene expression, a severe loss of neural synapses in the larval brain, and high levels of larval mortality. The larvicidal activities of yeast interfering RNA larvicides were retained following heat inactivation and drying of the yeast into user-friendly tablet formulations that induced up to 100% larval mortality in laboratory trials.
Ready-to-use dried inactivated yeast interfering RNA larvicide tablets may someday be an effective and inexpensive addition to malaria mosquito control programmes and a valuable, biorational tool for addressing residual malaria transmission.
Although insecticide-treated nets (ITNs) and indoor residual spraying (IRS) have been the backbone for malaria vector control, resistance to insecticides used for these applications is a growing problem. Furthermore, these interventions cannot control mosquitoes that bite or rest outdoors . As residual transmission of malaria becomes increasingly problematic, there is renewed interest in the use of larval source management (LSM) for reduction of residual transmission. In the first half of the twentieth century, LSM was a large-scale and highly effective method for control of malaria. Although large-scale LSM programmes were disbanded and replaced by IRS with dichlorodiphenyltrichloroethane (DDT) in the latter part of the century, LSM is still a major component of integrated mosquito control programmes in some parts of the world . Moreover, LSM, unlike IRS and ITNs, can reduce the number of mosquitoes that enter houses and the number of outdoor-biting mosquitoes .
Larviciding, a form of LSM, involves the application of chemical or biological agents to water bodies for targeting of immature aquatic larvae and pupae before they become malaria vector mosquitoes. Integrated control programmes that included larviciding were successful in Tanzania, Sudan, and Mauritius [2, 3], and a recent study in Kenya demonstrated that long-lasting FourStar™ briquette larvicides significantly reduced mean densities of indoor- and outdoor-biting adult malaria vector mosquitoes . The World Health Organization (WHO) recommended that larviciding, when used as a supplement to ITNs and IRS in sub-Saharan Africa, is cost-effective for malaria control in urban settings where vector breeding sites are few, fixed, and findable . However, given the increase of reported insecticide resistance and rising concern for the negative effects of pesticides on non-target organisms, the current pesticide repertoire is faced with great challenges to sustainability . The identification of new, environmentally safe, cost-effective larvicides is critical if the current levels of larviciding are to be sustained or expanded.
Interfering RNA molecules represent a novel class of larvicides with untapped potential for sustainable mosquito control. Although RNA interference (RNAi) is beginning to attract attention in agricultural biotechnology communities [5,6,7], RNAi is still a largely unexplored approach for control of disease vector mosquitoes. The RNAi pathway is initiated by Dicer, which cleaves long pieces of double stranded RNA (dsRNA) into small interfering RNAs (siRNAs) which silence genes that are complementary in sequence. Most mosquito researchers use longer (300–400 bp) dsRNA molecules for RNAi. However, the short length (21–25 bp) of custom siRNAs and their short hairpin RNA (shRNA) counterparts facilitates the design of interfering RNA that targets mosquitoes, but not humans or other non-target organisms [8, 9]. siRNAs have facilitated our functional genetic characterization of mosquito larval development [10,11,12,13,14]. This investigation tested the hypothesis that short interfering RNA molecules can be utilized as larvicidal agents for control of Anopheles mosquitoes. The authors recently conducted a high throughput screen (MDS, in preparation) that resulted in the identification of > 100 mosquito siRNA larvicides. Here, the characterization of highly toxic interfering RNAs targeting three larval lethal mosquito genes identified in the screen, suppressor of actin (Sac1), leukocyte receptor complex member (lrc), and offtrack (otk), is described. The study then describes the bioengineering and testing of a Saccharomyces cerevisiae (baker’s yeast) system for delivery of these interfering RNA molecules to Anopheles gambiae mosquito larvae. The results of this investigation demonstrate that heat-inactivated dry yeast interfering RNA pellets targeting these genes induce severe defects in the mosquito central nervous system and up to 100% larval mortality.
The A. gambiae M strain (obtained from N. Besansky) and the Aedes aegypti Liverpool-IB12 (LVP-IB12; obtained from D. Severson) strain were used in these studies and maintained generally as described , except that an artificial membrane feeding system was used for delivery of sheep blood (HemoStat Laboratories, Dixon, CA) to adult female mosquitoes. The insects were reared in an insectary maintained at 26 °C, at ~ 80% humidity, and under a 12 h light/12 h dark cycle with 1 h crepuscular periods at the beginning and end of each light cycle.
Identification of larvicidal siRNAs
An siRNA larvicide screen led to the identification of siRNAs Sac1.1 and Sac1.91 which correspond to Sac1 (AGAP000891), lrc.2 and lrc.51 which target lrc (AGAP008903), and otk.16 and otk.94 which correspond to otk (AGAP011489). For the screen, custom siRNAs corresponding to Anopheles orthologs of a subset of Drosophila larval lethal genes  as well as a control siRNA  with no known target in An. gambiae were purchased from Integrated DNA Technologies. The sequences targeted by these siRNAs, are as follows:
Basic local alignment search tool (BLAST)  searches indicated that the siRNAs corresponding to Sac1, lrc, and otk lacked identical matches in Aedes mosquitoes, amphibians, birds, fish, fungi, humans, mammals, plants, and reptiles (Additional file 1). The screen involved a dual-testing approach that included microinjection of third instar larvae as well as soaking of first instar larvae, both of which were performed in duplicate. For injections, ~ 10 pmol custom screening siRNA were injected in a 30 nL volume per larva (n = 30/condition/replicate) using previously described methodology [18, 19]. siRNAs were simultaneously screened through delivery via larval soaking (per ), which permitted a second round of selection to identify siRNAs that are capable of killing mosquitoes early in larval development following only brief exposure to siRNA, which may better simulate field conditions. For soaking experiments, 20 first instar larvae/condition/replicate were exposed to 20 µL of 0.5 µg/µL siRNA for 4 h. Following siRNA treatment, larvae were reared and lethality evaluated per the WHO  larvicide testing guidelines. The mortality of larvae treated with siRNA via soaking or microinjection was compared to control-treated animals using the Fisher’s exact test . In the larval screen, as well as all other larvicide assays reported here, larvae that were not treated with larvicidal or control RNA and fed a normal laboratory diet were reared in parallel. No significant differences in the mortality of control-treated vs. non-treated larvae were detected in any of the assays conducted in this investigation. The results for control-treated larvae are reported herein.
Bacteria interfering RNA larvicide preparation and feeding
Heat-killed non-pathogenic Escherichia coli expressing dsRNAs of interest were constructed and fed to larvae beginning in the first instar (L1) stage using the general protocol of Whyard et al. , which was adapted for use in An. gambiae. Strain HT115-DE3, obtained from the Caenorhabditis Genetics Center (which is funded by the NIH Office of Research Infrastructure Programs, P40 OD010440), was used in these studies. Bacteria were transformed with the dsRNA transcription plasmid pL4440 (deposited at Addgene by Andrew Fire; plasmid # 1654), which contains forward and reverse T7 polymerase binding sites that flank a multiple cloning site in which DNA corresponding to the Sac1.1, lrc.2, or otk.16 siRNA target sequences had been cloned. This permitted inducible expression of dsRNA in E. coli, which were prepared and fed to larvae as discussed , with liver powder being substituted for ground fish food (Doctors Foster and Smith, Stable Diet, Rhinelander, Wisconsin). Escherichia coli that had been transformed with GFP:L4440, which was deposited at Addgene by Guy Caldwell (Addgene plasmid # 11335) and expresses dsRNA corresponding to GFP, was used as a control feeding strain in these experiments. Data were compiled from at least two biological replicate experiments, each with four replicate cups bearing 20 animals for each treatment (n = 240 control-treated larvae, 240 lrc.2-treated larvae, and 160 otk.16-treated larvae) and assessed by ANOVA with Tukey’s multiple comparison test.
Yeast interfering RNA larvicide preparation and feeding
shRNA-encoding DNA oligonucleotides corresponding to the Sar1.1, lrc.51, otk.16, and control siRNA target sequences were custom synthesized by Invitrogen Life Technologies. These shRNA expression cassettes were cloned into the non-integrating pRS426 GPD yeast shuttle vector, which has a URA3 marker and permits constitutive expression of inserts cloned downstream of a GPD promoter . Following sequencing to confirm the hairpin expression cassette sequences, the plasmids were transformed into S. cerevisiae strain BY4742  (genotype MATα his3Δ1 leu2Δ0 lys2Δ0 ura3Δ0). Transformants were selected by checking for growth on minimal media lacking uracil. Following selection, the yeast was grown to an OD600 of 3.0 under standard conditions in synthetic media. For gel-coated formulations, the Whyard et al.  procedure for bacterial pellet preparation was used in conjunction with a 50 mL yeast culture. For preparation of dried tablet formulations, 50 mL of yeast culture was transferred to 50 mL conical tubes and pelleted by centrifugation for 20 min at 4000 rpm (Eppendorf 5810R plus), and the supernatant (culture media) was discarded. For heat inactivation, the pellet was placed in a 70 °C water bath for 5 min. The yeast pellet was then placed into a 2 mL tube which contained 10 mg of fish food and centrifuged for 1 min at ~ 13.2 rpm (Eppendorf, 5415D). The supernatant was discarded, and the open tubes were placed in an incubator at 30 °C for 48 h to permit evaporation of the remaining media. The dried tablets were stored in capped microfuge tubes at – 20 °C. The final weight of each yeast tablet averaged 95 mg, including 10 mg of fish food and 85 mg of yeast (~ 1.6 × 1010 cells).
For each replicate, agarose-gel coated yeast pellets were divided into three portions, with each portion fed daily to 20 larvae beginning in L1 for 3 days. For dried yeast formulations, at the beginning of each experiment, one control or experimental tablet was placed in a container with 20 L1 animals. The larval bioassays were performed in 500 mL plastic cups containing 50 mL of water. For the gel-coated live yeast experiments, data were compiled from two biological replicate experiments, each with three replicates per condition and 20 larvae per replicate for a total n of 120 larvae/condition. For the gel-coated inactivated yeast experiments, data were compiled from three biological replicate experiments, each with three replicates per condition and 20 larvae per replicate for a total n of 180 larvae/condition. For the dried inactivated yeast tablet experiments, data were compiled from three biological replicate experiments with four replicates per condition and 20 animals per replicate (n = 240 larvae/condition). Yeast interfering RNA larvicide data were assessed by ANOVA with Tukey’s multiple comparison test.
Whole mount in situ hybridization and immunohistochemistry
Riboprobes corresponding to the Sac1, lrc, and otk genes were synthesized according to the Patel  protocol, and in situ hybridization experiments were performed in duplicate according to the Haugen et al.  protocol. At the initiation of tissue fixation, larvae were living. Stained tissues were mounted, analysed, and imaged using a Zeiss Axioimager equipped with a Spot Flex camera. For quantification of transcripts, mean gray values were calculated for digoxigenin-labeled transcript signal in control or experimental brains. For each probe, the results from three biological replicate experiments were compiled (n = 40 control-treated brains/per probe, n = 85 Sac1.1-treated brains, n = 80 lrc.51-treated brains, and n = 80 otk.16-treated brains). A t test was used to analyse transcript quantification data.
Immunohistochemical staining experiments were performed as described [28, 29] using the nuclear stain TO-PRO-3 iodide (Molecular Probes, Eugene, OR) and mAb 3C11, which recognizes the Synapsin-1 cleaved fragment . mAb 3C11 was deposited by E. Buchner at the Developmental Studies Hybridoma Bank, a facility created by the NICHD of the NIH and maintained at The University of Iowa. Larvae were still living at the initiation of tissue fixation. Following processing, the tissues were mounted and then imaged at the IUSM Flow Cytometry and Imaging Core facility using a Zeiss 710 confocal microscope and Zen software. FIJI ImageJ and Adobe Photoshop CC 2014 software were used to analyse the images. Three biological replicate experiments were performed, with a total of 25 brains evaluated per condition.
Sac1, otk and lrc are mosquito larval lethal genes
A dual-screening approach was employed to evaluate siRNAs corresponding to Anopheles orthologs of Drosophila melanogaster larval lethal genes  for larvicidal activity. siRNAs were screened both through microinjection of third instar larvae (Fig. 1a) as well as through 4 h soaking treatment of first instar larvae (Fig. 1b). Microinjection of siRNA Sac1.1, which corresponds to the Sac1 gene, resulted in 42 ± 4% larval mortality (Fig. 1a; p < 0.01 vs. control siRNA injected animals). siRNA lrc.2, which targets a sequence in the lrc gene, resulted in significant 42 ± 2% mortality following injection (Fig. 1b; p < 0.05 vs. control), while injection of siRNA otk.16, which corresponds to otk, yielded 40 ± 4% larval mortality (p < 0.001 vs. control). siRNAs Sac1.1, lrc.2, and otk.16 also displayed significant larvicidal activity (p < 0.01 vs. control) in short-term exposure soaking experiments conducted with first instar larvae, inducing 45 ± 12, 29 ± 6 and 28 ± 5% larval mortality, respectively (Fig. 1b). These experiments indicated that exposure to the siRNAs either early (L1) or later (L3) in larval development can result in death.
The larvicidal activity of these interfering RNAs was further confirmed by feeding larvae heat-killed E. coli prepared as described by Whyard et al.  that had been engineered to express dsRNA corresponding to the Sac1.1, lrc.2, and otk.16 siRNA target sequences. These experiments, in which bacteria interfering RNA larvicides Sac1.1, lrc.2, and otk.16 induced 43 ± 1, 99 ± 0, and 84 ± 1% death (Fig. 1c), further demonstrated the larvicidal capacity of these interfering RNA molecules. Silencing experiments were also conducted with siRNAs corresponding to additional target sequences in the Sac1, lrc, and otk genes. Injection of siRNA Sac1.91, which corresponds to an alternative target site in Sac1, induced 29 ± 2% larval mortality (p < 0.05 vs. control siRNA). siRNA lrc.51, which targets an alternate site in lrc, resulted in 55 ± 1% death (p < 0.001 vs. control siRNA) following soaking treatment. Injection of siRNA otk.94, which corresponds to an alternative target site in otk, induced 40 ± 10% mortality (p < 0.001 vs. control siRNA). These results indicate that targeting alternative sites in Sac1, lrc, or otk induces larval death, providing further evidence that these genes are required for larval survival.
Exploration of yeast interfering RNA delivery systems
The results from the siRNA larval lethal screen and bacterial short dsRNA larvicide studies supported the hypothesis that yeast expressing shRNA that targets larval lethal genes could be used as larvicides. In initial experiments, shRNA corresponding to the Sac1.1, otk.16, or control siRNA target sequence was constitutively expressed from a non-integrating multi-copy yeast shuttle plasmid that was transformed into S. cerevisiae. This yeast strain, as well as a control yeast strain expressing shRNA with no known target in An. gambiae, was initially fed to larvae in an agarose gel-covered formulation (Fig. 2a) using methodology that was comparable to the preparation of bacterial interfering RNA larvicides. Since both live and heat-inactivated bacteria can induce mosquito death , both live and dead yeast covered in agarose were tested. While control-fed larvae survived, gel-coated live yeast larvicides Sac1.1 and otk.16 killed 80 ± 4 (Fig. 2a; p < 0.001 vs. control) and 83 ± 4% of mosquitoes (Fig. 2a; p < 0.001 vs. control), respectively. Heat-inactivated gel-coated yeast Sac1.1 induced 86 ± 1% mortality (Fig. 2b; p < 0.001 vs. control), while heat-inactivated gel-coated yeast otk.16 induced 84 ± 1% mortality (Fig. 2b; p < 0.001 vs. control). No significant differences were observed in the larvicidal capacity of live vs. heat-inactivated yeast interfering RNA larvicides (Fig. 2a vs. b). Heat-inactivated Sac1.1 and otk.16 yeast fed to A. aegypti larvae, in which the target sequences of these interfering RNAs are not conserved, did not induce larval death (Additional file 2; p = 0.66).
Dried inactivated yeast interfering RNA larvicide tablets induce significant larval death
Although agarose-coated yeast larvicides induced high mortality rates (Fig. 2), these formulations are sticky and non user-friendly. Also, the water in containers treated with the gel-coated yeast becomes cloudy, which may not be desired by prospective users. To circumvent these issues, dried tablets of inactivated yeast (Fig. 3a), which are comparable in appearance to yeast nutritional tablets sold as human dietary supplements, were therefore prepared and evaluated. This formulation is easier to handle, does not cloud the water in treated containers, and is readily consumed by Anopheles larvae. Treatment of 50 mL water containing 20 larvae with a 95 mg dried tablet of yeast interfering RNA larvicide Sac1.1 induced 89 ± 1% larval mortality (Fig. 3b; p < 0.001 vs. control). Dried yeast interfering RNA larvicide otk.16 induced 89 ± 1% larval mortality (Fig. 3b; p < 0.001 vs. control). Yeast expressing shRNA corresponding to the lrc.51 target sequence was also prepared, and these tablets induced 100 ± 0% larval mortality (Fig. 3b; p < 0.001 vs. control). These results demonstrated that dried inactivated yeast interfering RNA larvicide tablets have highly significant larvicidal activity.
Yeast interfering RNA larvicide-mediated silencing of Sac1, otk, or lrc disrupts neural synapses in the larval brain
In D. melanogaster, Sac1 encodes phosphatidylinositol phosphatase, which functions to dephosphorylate phosphatidylinositol 4-phosphate for generation of phosphatidylinositol and acts as an axon guidance regulator . The D. melanogaster otk gene encodes a member of the Tyrosine protein kinase superfamily which functions as a neural cell adhesion molecule to regulate axon guidance [32, 33]. The D. melanogaster CG6700 gene is an lrc ortholog and encodes a conserved C-terminal SAC3/GANP domain-containing protein member of the dystroglycan–dystrophin complex [34,35,36]. CG6700 was listed in a catalog of genes likely to function in synapse assembly and function , but its function in this capacity remained to be tested. Given the reported neural functions of the Sac1, lrc, and otk Drosophila orthologs, the functions of these genes were assessed in the mosquito brain (Fig. 4). Detection (Fig. 4a2 vs. a1) and quantification (Fig. 4a3) of Sac1 transcript levels in the L4 larval brain demonstrated that ingestion of yeast interfering larvicide Sac1.1 resulted in 85 ± 5% reduction of Sac1 transcripts (p < 0.001). Detection (Fig. 4b2 vs. b1) and quantification (Fig. 4b3) of L4 larval brain lrc transcripts showed that ingestion of yeast interfering RNA larvicide lrc.51 resulted in 88 ± 6% reduction of lrc transcripts. Likewise, detection (Fig. 4c2 vs. c1) and quantification (Fig. 4c3) of otk transcripts in the L4 larval brain indicated that ingestion of yeast interfering RNA larvicide otk.16 resulted in 83 ± 5% reduction of otk transcripts.
Detection of Synapsin expression (with mAb 3C11 ), a marker of active neural synapses in multiple arthropod species , was used to assess synaptic activity in the brains of animals fed with these yeast interfering RNA larvicides. Synapsin expression was severely reduced in the synaptic neuropiles of animals fed with yeast interfering RNA larvicides Sac1.1 (Fig. 5b1, b2 vs. control-fed animals in a1, a2), lrc.51 (Fig. 5c1, c2 vs. a1, a2), and otk.16 (Fig. 5d1, d2 vs. a1, a2). These severe neural phenotypes are likely to be primary causes of larval death in animals fed with yeast interfering RNA larvicides targeting these genes.
Numerous studies have demonstrated that target gene silencing through RNAi can promote insect death . For example, Baum et al.  engineered transgenic corn plants expressing dsRNA targeting the western corn rootworm Diabrotica virgifera virgifera. dsRNA insecticidal corn targeting this species was recently registered by the US Environmental Protection Agency , which deemed that this intervention meets the regulatory standards described in the Federal Insecticide, Fungicide, and Rodenticide Act . Likewise, Whyard et al.  showed that Tribolium castaneum, Acyrthosiphon pisum, and Manduca sexta were killed when fed species-specific dsRNA targeting vATPase. The sequence specificity of RNAi facilitated their design of dsRNAs that targeted specific chosen insects, but which did not kill non-target insects, including closely related insect species . Similarly, this study designed yeast interfering RNA larvicides with target sequences in Anopheles larval lethal genes that are not perfectly conserved in other organisms (Additional file 1) and which failed to kill A. aegypti (Additional file 2). Of course, the ability of an siRNA to have off-target effects is complicated . It is difficult to predict, on the basis of sequence information alone, whether these yeast interfering RNA larvicides could impact gene expression in non-target organisms , and it will be important to conduct more detailed toxicity studies on these larvicides. However, in general, interfering RNA pesticides are believed to be much safer than chemical pesticides . MonSanto  concluded, in an extensive evaluation of RNA molecules prepared for the United States Environmental Protection Agency, that RNA based products are an important technology with great promise for pest mitigation applications while presenting an overwhelmingly desirable safety profile, particularly when compared to conventional pesticides. Moreover, although many had questioned whether interfering RNAs were sufficiently stable for field applications, dsRNA stability has actually been reported to be quite high [44, 45]. These and other studies suggest that RNAi can be exploited to control insect agricultural pests.
RNAi has been used extensively for functional analysis of mosquito genes [10,11,12,13,14]. However, RNAi has not yet emerged as a method for mosquito control. The results of this investigation, in which a number of larval lethal genes to be targeted and an effective delivery system for interfering RNAs targeting these genes were identified, suggest that the addition of RNAi pesticides to integrated mosquito control programmes may be feasible and beneficial. Through the identification of multiple larval lethal genes and target sites in these genes, including those described here and additional RNAi targets in the An. gambiae genome that have been discovered and tested, the authors hope to build an arsenal of interfering RNAs that can be used to combat resistance to traditional chemical pesticides. This arsenal can also be used to combat future resistance that might develop to any single interfering RNA pesticide.
The broad application of RNAi for pest control is dependent upon production of dsRNA in an economically feasible, scalable, and sustainable fashion. dsRNA manufacture has traditionally relied on expensive, carbon-intensive chemical synthesis, resulting in high costs [5, 6] and a perception that use of RNAi for mosquito control would be prohibitively expensive. Additionally, a perceived high operational cost and the complexity of Anopheles larviciding in general has deterred some mosquito control programmes from adopting LSM strategies for malaria vector control . The use of ready-to-use yeast interfering RNA larvicide tablets, which are a user-friendly economically feasible biorational alternative to conventional larvicides may help to address these concerns. While Pichia pastoris has been used for expression of recombinant DNA and dsRNA to target Aedes [46, 47], in this investigation, we opted to use S. cerevisiae, for which many mutant strains and plasmid constructs exist. Interfering RNA was affordably propagated through cultivation of the yeast. The first three Anopheles interfering RNA larvicides generated in S. cerevisiae, Sac1.1, lrc.51, and otk.16 (Figs. 2, 3), effectively killed mosquitoes, with lrc.51 inducing 100% larval mortality. As with bacteria , the larvicides retained full activity after the yeast was heat-killed (Fig. 2), which circumvents concerns for the introduction of live genetically modified organisms for mosquito control.
Saccharomyces cerevisiae has been cultivated worldwide for thousands of years, and this technology can be adapted to resource-limited countries with constrained infrastructures. Moreover, dried yeast can be packaged and shipped in both active (live) or inactive (dead) forms, which will facilitate regional distribution. Yeast production is readily scaled to industry-sized cultures, and so commercialization of this intervention is feasible. S. cerevisiae, which is non-toxic to humans, is already used globally in food and alcoholic beverage preparation. Dried inactive yeast is sold commercially as a dietary supplement and is available in tablet or flake formulations. It is anticipated that heat-inactivated yeast interfering RNA, which demonstrated high larvicidal activities in this investigation, could be prepared in bulk and distributed in these ready-to-use dried formulations.
Given the many benefits of the yeast system, the encouraging results reported in this study, as well as a recent study in the agricultural pest Drosophila suzukii , support the pursuit of proof-of-concept semi-field evaluation of yeast interfering RNA larvicides. To this end, semi-field trials with heat inactivated yeast interfering RNA larvicides are planned. This critical next phase of the project will facilitate evaluation of the efficacy, feasibility, and acceptance of introducing biorational yeast interfering RNA larvicides into integrated vector mosquito control programmes. Given that yeast, a strong odorant attractant for larvae, can act as a larval bait , it is likely that yeast interfering RNA pellets could be used to treat volumes of water that are much larger than those used in the present investigation, and this will need to be assessed in the field. It would also be interesting to test additional yeast formulations in the field. For example, it is possible that some species of Anopheles larvae may more readily ingest yeast interfering RNA flakes that float at the water surface, and this could become critical in the field, where competing food sources are available to larvae. Finally, in addition to assessing the impacts of yeast interfering RNA larvicides on the densities of juvenile and adult mosquitoes in the field, it will be important to examine the best settings for the use of these larvicides, if they can be used for control of other malaria vector mosquitoes, and ultimately to demonstrate that the larvicides can effectively reduce the number of malaria cases.
In summary, new vector control tools to address residual malaria transmission are vitally needed. The laboratory trials conducted in this investigation demonstrated that yeast expressing shRNA corresponding to An. gambiae larval lethal genes induce up to 100% larval mortality. These yeast interfering RNA larvicides retain larvicidal activity following drying and heat-inactivation of the yeast into ready-to-use tablet formulations. Dried inactivated yeast interfering RNA larvicide tablets could someday be an effective, inexpensive, biorational addition to malaria mosquito control programmes and a valuable tool for combating residual malaria transmission.
analysis of variance
basic local alignment search tool
double stranded RNA
Environmental Protection Agency
indoor residual spraying
insecticide treated nets
- lrc :
leukocyte receptor complex member
- otk :
short hairpin RNA
small interfering RNA
- Sac1 :
suppressor of actin
World Health Organization
WHO. World malaria report 2016. Geneva: World Health Organization; 2016.
WHO. Larval source management: a supplementary measure for malaria vector control: an operational manual. Geneva: World Health Organization; 2013.
Fillinger U, Lindsay SW. Larval source management for malaria control in Africa: myths and reality. Malar J. 2011;10:353.
Afrane YA, Mweresa NG, Wanjala CL, Gilbreath Iii TM, Zhou G, Lee MC, Githeko AK, Yan G. Evaluation of long-lasting microbial larvicide for malaria vector control in Kenya. Malar J. 2016;15:577.
Yu N, Christiaens O, Liu J, Niu J, Cappelle K, Caccia S, Huvenne H, Smagghe G. Delivery of dsRNA for RNAi in insects: an overview and future directions. Insect Sci. 2013;20:4–14.
Zhang H, Li HC, Miao XX. Feasibility, limitation and possible solutions of RNAi-based technology for insect pest control. Insect Sci. 2013;20:15–30.
EPA. Pesticide product with new active ingredients dsRNA transcipt comprising a DvSnf7 inverted repeat sequence derived from Diabrotica virgifera virgifera and Bt Cry3Bb1 protein and the genetic material necessary for their production (vector PV-ZMIR10871) in MON 87411 Corn (OECD Unique Identifier MON-87411-9)—FIFRA. 2015. https://www.noticeandcomment.com/Final-Regulatory-Decision-for-New-Active-Ingredients-Double-stranded-Ribonucleic-Acid-Transcript-Comprising-fn-316831.aspx. Accessed Nov 2015.
Qiu S, Adema CM, Lane T. A computational study of off-target effects of RNA interference. Nucleic Acids Res. 2005;33:1834–47.
Moffat J, Reiling JH, Sabatini DM. Off-target effects associated with long dsRNAs in Drosophila RNAi screens. Trends Pharmacol Sci. 2007;28:149–51.
Mysore K, Flannery EM, Tomchaney M, Severson DW, Duman-Scheel M. Disruption of Aedes aegypti olfactory system development through chitosan/siRNA nanoparticle targeting of semaphorin-1a. PLoS Negl Trop Dis. 2013;7(5):e2215.
Mysore K, Andrews E, Li P, Duman-Scheel M. Chitosan/siRNA nanoparticle targeting demonstrates a requirement for single-minded during larval and pupal olfactory system development of the vector mosquito Aedes aegypti. BMC Dev Biol. 2014;14:9.
Mysore K, Flannery E, Leming MT, Tomchaney M, Shi L, Sun L, O’Tousa JE, et al. Role of semaphorin-1a in the developing visual system of the disease vector mosquito Aedes aegypti. Dev Dyn. 2014;243:1457–69.
Mysore K, Sun L, Tomchaney M, Sullivan G, Adams H, Piscoya AS, et al. siRNA-mediated silencing of doublesex during female development of the dengue vector mosquito Aedes aegypti. PLoS Negl Trop Dis. 2015;9:e0004213.
Tomchaney M, Mysore K, Sun L, Li P, Emrich SJ, Severson DW, et al. Examination of the genetic basis for sexual dimorphism in the Aedes aegypti (dengue vector mosquito) pupal brain. Biol Sex Differ. 2014;5:10.
Clemons A, Mori A, Haugen M, Severson DW, Duman-Scheel M. Culturing and egg collection of Aedes aegypti. Cold Spring Harb Protoc. 2010;pdb prot5507.
St Pierre SE, Ponting L, Stefancsik R, McQuilton P, FlyBase Consortium. FlyBase 102-advanced approaches to interrogating FlyBase. Nucleic Acids Res. 2014;42:D780–8.
Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215:403–10.
Blitzer EJ, Vyazunova I, Lan Q. Functional analysis of AeSCP-2 using gene expression knockdown in the yellow fever mosquito, Aedes aegypti. Insect Mol Biol. 2005;14:301–7.
Clemons A, Haugen M, Le C, Mori A, Tomchaney M, Severson DW, Duman-Scheel M. siRNA-mediated gene targeting in Aedes aegypti embryos reveals that frazzled regulates vector mosquito CNS development. PLoS ONE. 2011;6:e16730.
Singh AD, Wong S, Ryan CP, Whyard S. Oral delivery of double-stranded RNA in larvae of the yellow fever mosquito, Aedes aegypti: implications for pest mosquito control. J Insect Sci. 2013;13:69.
WHO. Guidelines for laboratory and field testing of mosquito larvicides. Geneva: World Health Organization; 2005.
Fisher RA. Statistical methods for research workers. Edinburgh: Oliver and Boyd; 1925.
Whyard S, Erdelyan CN, Partridge AL, Singh AD, Beebe NW, Capina R. Silencing the buzz: a new approach to population suppression of mosquitoes by feeding larvae double-stranded RNAs. Parasit Vectors. 2015;8:96.
Mumberg D, Muller R, Funk M. Yeast vectors for the controlled expression of heterologous proteins in different genetic backgrounds. Gene. 1995;156:119–22.
Winzeler EA, Shoemaker DD, Astromoff A, Liang H, Anderson K, Andre B, et al. Functional characterization of the S. cerevisiae genome by gene deletion and parallel analysis. Science. 1999;285:901–6.
Patel NH. In situ hybridization to whole mount Drosophila embryos. In: Krieg PA, editor. A laboratory guide to RNA: isolation, analysis, and synthesis. New York: Wiley-Liss; 1996. p. 357–70.
Haugen M, Tomchaney M, Kast K, Flannery E, Clemons A, Jacowski C, et al. Whole-mount in situ hybridization for analysis of gene expression during Aedes aegypti development. Cold Spring Harb Protoc. 2010(10). https://doi.org/10.1101/pdb.prot5509.
Clemons A, Flannery E, Kast K, Severson D, Duman-Scheel M. Immunohistochemical analysis of protein expression during Aedes aegypti development. Cold Spring Harb Protoc. 2010(10). https://doi.org/10.1101/pdb.prot5510
Mysore K, Flister S, Muller P, Rodrigues V, Reichert H. Brain development in the yellow fever mosquito Aedes aegypti: a comparative immunocytochemical analysis using cross-reacting antibodies from Drosophila melanogaster. Dev Genes Evol. 2011;221:281–96.
Klagges BR, Heimbeck G, Godenschwege TA, Hofbauer A, Pflugfelder GO, Reifegerste R, et al. Invertebrate synapsins: a single gene codes for several isoforms in Drosophila. J Neurosci. 1996;16:3154–65.
Lee S, Kim S, Nahm M, Kim E, Kim TI, Yoon JH, Lee S. The phosphoinositide phosphatase Sac1 is required for midline axon guidance. Mol Cells. 2011;32:477–82.
Pulido D, Campuzano S, Koda T, Modolell J, Barbacid M. Dtrk, a Drosophila gene related to the trk family of neurotrophin receptors, encodes a novel class of neural cell adhesion molecule. EMBO J. 1992;11:391–404.
Winberg ML, Tamagnone L, Bai J, Comoglio PM, Montell D, Goodman CS. The transmembrane protein Off-track associates with Plexins and functions downstream of Semaphorin signaling during axon guidance. Neuron. 2001;32:53–62.
Dietzl G, Chen D, Schnorrer F, Su KC, Barinova Y, Fellner M, et al. A genome-wide transgenic RNAi library for conditional gene inactivation in Drosophila. Nature. 2007;448:151–6.
Jankovics F, Henn L, Bujna A, Vilmos P, Kiss N, Erdelyi M. A functional genomic screen combined with time-lapse microscopy uncovers a novel set of genes involved in dorsal closure of Drosophila embryos. PLoS ONE. 2011;6:e22229.
Kucherenko MM, Pantoja M, Yatsenko AS, Shcherbata HR, Fischer KA, Maksymiv DV, et al. Genetic modifier screens reveal new components that interact with the Drosophila dystroglycan–dystrophin complex. PLoS ONE. 2008;3:e2418.
Pazos Obregon F, Papalardo C, Castro S, Guerberoff G, Cantera R. Putative synaptic genes defined from a Drosophila whole body developmental transcriptome by a machine learning approach. BMC Genomics. 2015;16:694.
Baum JA, Bogaert T, Clinton W, Heck GR, Feldmann P, Ilagan O, et al. Control of coleopteran insect pests through RNA interference. Nat Biotechnol. 2007;25:1322–6.
EPA. Pesticide product with new active ingredients dsRNA transcript comprising a DvSnf7 inverted repeat sequence derived from Diabrotica virgifera virgifera and Bt Cry3Bb1 protein and the genetic material necessary for their production (vector PV-ZMIR10871) in MON 87411 Corn (OECD Unique Identifier MON-87411-9)—FIFRA. 2015. https://www.noticeandcomment.com/EPA-HQ-OPP-2014-0293-fdt-52976.aspx. Accessed July 2017.
FIRFA. Summary of the Federal insecticide, fungicide, and rodenticide act. 2015. http://www.epa.gov/laws-regulations/summary-federal-insecticide-fungicide-and-rodenticide-act. Accessed Nov 2015.
Whyard S, Singh AD, Wong S. Ingested double-stranded RNAs can act as species-specific insecticides. Insect Biochem Mol Biol. 2009;39:824–32.
Jackson AL, Linsley PS. Recognizing and avoiding siRNA off-target effects for target identification and therapeutic application. Nat Rev Drug Discov. 2010;9:57–67.
MonSanto. Docket ID: EPA-HQ-OPP-2013-0485. 2014. https://www.apsnet.org/members/outreach/ppb/Documents/MonsantopostedwrittencommentJan2014.pdf. Accessed June 2015.
Li H, Guan R, Guo H, Miao X. New insights into an RNAi approach for plant defence against piercing-sucking and stem-borer insect pests. Plant Cell Environ. 2015;38:2277–85.
San Miguel K, Scott JG. The next generation of insecticides: dsRNA is stable as a foliar-applied insecticide. Pest Manag Sci. 2016;72:801–9.
Borovsky D, Nauwelaers S, Van Mileghem A, Meyvis Y, Laeremans A, Theunis C, et al. Control of mosquito larvae with TMOF and 60 kDa Cry4Aa expressed in Pichia pastoris. Pestycydy/Pesticides. 2011;1:5–15.
Van Ekert E, Powell CA, Shatters RG Jr, Borovsky D. Control of larval and egg development in Aedes aegypti with RNA interference against juvenile hormone acid methyl transferase. J Insect Physiol. 2014;70:143–50.
Murphy KA, Tabuloc CA, Cervantes KR, Chiu JC. Ingestion of genetically modified yeast symbiont reduces fitness of an insect pest via RNA interference. Sci Rep. 2016;6:22587.
KM acquired, analysed, and interpreted the yeast larvicide data and assisted with manuscript preparation. LH assisted with study design, acquired, and analysed the yeast larvicide data. LS performed and helped analyse the microinjection screen and assisted with mosquito rearing. EIH and JSR performed and helped analyse the soaking screen and assisted with mosquito rearing. NDS performed and analysed the Aedes aegypti studies. YC prepared the yeast used in these studies and assisted with data analysis. KE, DWS and NW assisted with study design, data analysis, and interpretation. MDS prepared the manuscript, conceived of the study, designed experiments, and assisted with cloning, data analysis and interpretation. All authors read and approved the final manuscript.
Thanks to Nicole Achee, John Grieco, Neil Lobo, and our colleagues in the Eck Institute for Global Health for useful discussions.
MDS, KKE, NW, and DWS have filed a patent application.
Availability of data and materials
All data generated or analysed during this study are included in this published article.
Consent for publication
Ethics approval and consent to participate
This work was funded by Bill and Melinda Gates Grand Challenges and Explorations Grant OPP ID # OPP1129038 and an Indiana University School of Medicine Ralph W. and Grace M. Showalter Research Trust Fund award to MDS. The funding sources were not involved in study design, data collection and interpretation, or the decision to submit the work for publication.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Additional file 1. Lack of siRNA larvicide target site conservation in non‐target organisms. Summary of Blast search results.
Additional file 2. A lack of Sac1.1 and otk.16 yeast interfering larvicide activity in A. aegypti larvae. Graph depicting results from larvicide trials that demonstrated a lack of larvicidal activity for yeast interfering RNA larvicides Sac1.1 and otk.16 in A. aegypti larvae.
About this article
Cite this article
Mysore, K., Hapairai, L.K., Sun, L. et al. Yeast interfering RNA larvicides targeting neural genes induce high rates of Anopheles larval mortality. Malar J 16, 461 (2017). https://doi.org/10.1186/s12936-017-2112-5
- Saccharomyces cerevisiae