We thank Drs. Anthony Cornel and Laura Norris at UC Davis and Dr. Katharina Kreppel at the University of Glasgow for providing mosquito specimens from Tanzania. We thank Ms.&#160;Smita Das and Dr. Douglas Norris from Johns Hopkins School of Public Health for sharing mosquito samples from Zambia. We also thank Mr. Lee V. Millon at the Veterinary Genetics Laboratory for training on assay design. This work was supported by the National Institute of Health grant R01AI 078183 and R21AI062929.

1. PCR Amplification
<ol>
	<li>Mix all the PCR primers (See supplemental Table S1) in a 1.5ml microtube. Each SNP has two primers (forward and reverse). Ensure that the stock concentration of each PCR primer is kept at 100 &#956;M. Make enough primer mix for 500-1,000 reactions to reduce pipetting error and time at the bench (See supplemental Table S2). If desired, prepare aliquots for 100-200 reactions per tube and store at -20&#176;C.</li>
	<li>Prepare PCR cocktail as described in the manufacturer&#8217;s protocol (Table 1). The volume for 96 reactions includes an overhang of 20%. Vortex the tube containing the PCR cocktail lightly and centrifuge for 30 sec&#160;at 2,000 x g.</li>
	<li>Dispense 3 &#956;l&#160;of the PCR cocktail into each well of a non-skirted 96 well plate. A repeater pipette can save time for this process.</li>
	<li>Add 2 &#956;l of the appropriate genomic DNA of mosquitoes in each well. 
	NOTE: Process of obtaining genomic DNA from mosquito tissues (head/thorax, abdomen or whole body) is described in other literatures29-32. Choose an appropriate DNA extraction protocol to differentiate those with Plasmodium in the blood (abdomen) from infective mosquitoes (Plasmodium in the head/thorax). We typically use DNA extracted from body parts (head/thorax or abdomen) of mosquitoes, so DNA concentration varies from 0.05-2ng/&#956;l. Although the total DNA input is lower than the manufacturer&#8217;s recommendation (5-10ng/rxn), we typically get robust SNP calls from 98% of DNA samples without whole genome amplification.</li>
	<li>Seal the plate, gently mix or vortex, and centrifuge for 1 min&#160;at 370 x g.</li>
	<li>Use the following thermocycler protocol to carry out PCR amplification: (1) 94&#176;C for 2 min, (2) 94&#176;C for 30 sec, (3) 56&#176;C for 30 sec, (4) 72&#176;C for 1 min, (5) repeat step (2)-(4) for 45 cycles, (6) 72&#176;C for 1 min, and 4&#176;C hold.</li>
</ol>
2. SAP Treatment
<ol>
	<li>Prepare the SAP enzyme solution in a 96 well plate (See Table 2). Process 96 samples in a plate. The volume for 96 reactions includes an overhang of 20%.</li>
	<li>Vortex the tube of SAP enzyme solution lightly and centrifuge for 30 sec&#160;at 2,000 x g. Dispense 2 &#956;l of the SAP enzyme solution into each well. Again, a repeater pipette can save time for this process.</li>
	<li>Seal the plate, gently mix or vortex, and centrifuge for 1 min&#160;at 370 x g. Incubate the plate as follows: (1) 37&#176;C for 40 min, (2) 85&#176;C for 5 min&#160;to inactivate the enzyme, (3) 4&#176;C hold. At completion of this step, store the plate at -20&#176;C before continuing. Process the stored plate within 2 weeks.</li>
</ol>
3. SNP Extension
<ol>
	<li>If the sample plate is frozen after SAP treatment, allow it to thaw to RT before proceeding.</li>
	<li>Prepare the extension primer mix (Supplemental Table S2). Each SNP has one extension primer. Keep the stock concentration of each extension primer at 500 &#956;M. Optionally, aliquot for 100-200 reactions per tube and store at -20&#176;C.</li>
	<li>Prepare extension mix as described in Table 3. The 96 reaction volume includes an overhang of 20%.</li>
	<li>Vortex the tube of extension cocktail lightly and centrifuge for 30 sec&#160;at 2,000 x g. Dispense 2 &#956;l of the extension cocktail into each well. Again, a repeater pipette can save time for this process.</li>
	<li>Seal the plate, gently mix or vortex, and centrifuge for 1 min&#160;at 370 x g. Thermocycle the plate as shown in Figure 1. At this point, proceed to mass spectrometry or store the plate at -20&#176;C up to 2 weeks.</li>
</ol>
4. Conditioning the SNP Extension Product to Optimize Mass Spectrometry Analysis
<ol>
	<li>If the sample plate is frozen after SNP extension, allow it to thaw to RT before proceeding.</li>
	<li>Transfer 15mg of resin from its container onto the dimple plate using an elongated spoon. Use the scraper to spread resin into the wells of the dimple plate. Sweep the scraper from side to side across the dimple plate to spread the resin. Make sure there is resin in each well.</li>
	<li>Scrape excess resin off the dimple plate using the scraper. Let the resin stand in the dimple plate for at least 20 min. While letting the resin stand in the dimple plate, add 41 &#956;l of HPLC grade water to each well of the sample plate.</li>
	<li>Gently place the sample plate upside-down, onto the dimple plate. Make sure the sample plate resets against the small rounded post of the dimple plate, which aligns the wells in the sample plate with the wells in the dimple plate.</li>
	<li>Holding the sample plate and the dimple plate together, gently flip them over so the resin falls out of the dimple plate into the wells of the sample plate. Tap the dimple plate so the resin falls out into the sample plate. Make sure all the resin in the dimple plate falls out into the sample plate wells. Centrifuge the plate at 3,200 x g for 30 sec.</li>
	<li>Rotate the sample plate on a rotator for 5 min&#160;at RT. Rotator must rotate the sample plate 360&#176; about the long axis.</li>
	<li>Centrifuge the sample plate at 3,200 x g for 5 min. After this step, store the sample plate at -20&#176;C up to 2 weeks before proceeding to the next step.</li>
</ol>
5. MALDI-TOF Mass Spectrometry
<ol>
	<li>Transfer the conditioned SNP extension product onto a bioarray such as SpectroCHIP as per manufacturer&#8217;s instructions. We use MassArray Nanodispenser for this step.</li>
	<li>Once the transfer is complete, define how assays and plates are to be set up in the assay database. Name the assay and plates such that each plate has unique identifier that links to specific assay design (Supplemental Table S3).</li>
	<li>After assay and plate have been defined, acquire spectra using a mass spectrometer.</li>
</ol>
6. Data Analysis
<ol>
	<li>Perform data analysis using a real-time PCR analysis data interpretation software such as Typer Analyzer or TyperViewer (Sequenom). Obtain data in .xml format which contains the sample layout, mass spectrogram for each well, the marker information including name, expected mass for each variant of the corresponding SNP, and any error or warning messages associated with each reaction. See Figure 2 for the resulting mass spectrogram.</li>
	<li>Carry out SNP genotype clustering analysis by setting the detection threshold (magnitude or signal to noise ratio) and tolerance/variance allowed for each genotype. Figure 3 shows an example of a 04707-KDR#2 SNP genotype clusters.</li>
	<li>Export the resulting SNP genotype calls into a spreadsheet program.</li>
</ol>

The authors have nothing to disclose.

The MDA is composed of five major steps: PCR amplification, shrimp alkaline phosphatase (SAP) reaction, SNP extension, extension product conditioning, and matrix-assisted laser desorption/ionization &#8211; time of flight (MALDI-TOF) mass spectrometry33-37. The first PCR amplification step amplifies DNA flanking each SNP so that enough template DNA will be available at the SNP extension step. The SAP reaction neutralizes unused dNTPs which can interfere with the following SNP extension step. SNP extension invo...

Anopheles arabiensis, Anopheles coluzzii and Anopheles gambiae are the major vectors responsible for malaria transmission in Africa1. These three species are morphologically indistinguishable2 and can only be distinguished by molecular assays3-9. In addition, there are many downstream assays routinely conducted to aid epidemiological and population genetics studies. These include (1) a genotyping assay for speciation islands10-12, (2) a genotyping assay recognizing non-synonymous SNPs in the 1014th amino acid codon position of para gene (the knock-down resistance, or kdr, SNP)13-18, (3) parasite detection PCR19-23, and (4) screening for host-specific DNA in mosquito midguts24,25.
We developed a multi-detection assay (MDA) that combines all these assays into a single multiplex reaction with the goal of analyzing epidemiologically important characteristics of malaria vectors in Africa. The MDA assay includes multiple markers for detecting (1) species (A. arabiensis, A. gambiae, A. coluzzii, or other (none of the three)), (2) insecticide resistance represented in kdr SNPs (both L1014Fand L1014S), (3) presence of two major malaria parasites, Plasmodium falciparum and P. vivax, and (4) blood source from one avian and six mammalian hosts.
Traditionally, these assays were conducted in separate polymerase chain reactions. When all these assays are done using a conventional PCR platform, it requires conducting 8-10 PCR reaction assays and accompanying gel electrophoresis steps. Each individual PCR reaction from preparation to documenting results takes 4-5 hr, while the MDA method presented here takes about 5 hr in totality. This is equivalent to a 90% savings in labor costs alone. The MDA presented here costs $5 per sample to genotype all 33 SNPs. This is considerably less expensive than the single agarose gel-based assays, which costs about $1.50 per sample. Assays detecting all the characteristics covered by the MDA would require a minimum of 8-10 separate agarose gel-based assays at a cost of $12-15 per sample. Moreover, the MDA greatly reduces the chance of generating a false positive or negative by utilizing at least three markers for each parasite or host source detection.
The platform we utilized is not limited to malaria vectors but can be used in a wide variety of applications such as medicine, veterinary medicine, and basic biology26-28. In-depth association studies or population genetics studies involving a large (in order of 100s) number of samples require cost-effective assays screening for multiple markers simultaneously. Most studies that utilize two or more separate PCR assays could implement the MDA for quicker results at a lower cost.

<table border="0" cellpadding="0" cellspacing="0" width="588">
	<tbody>
		<tr height="42">
			<td height="42" style="height:42px;width:216px;">Name of Material/ Equipment</td>
			<td style="width:87px;">Company</td>
			<td style="width:119px;">Catalog Number</td>
			<td style="width:167px;">Comments/Description</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">MassARRAY Analyzer Compact</td>
			<td style="width:87px;">Sequenom</td>
			<td style="width:119px;">MT9</td>
			<td>MALDI-TOF mass spectrometry for genomic applications to analyze nucleic acids.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">MassARRAY Nanodispenser</td>
			<td style="width:87px;">Sequenom</td>
			<td style="width:119px;">RS1000</td>
			<td>Transfers completed iPLEX reaction products to the SpectroCHIP</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:216px;">iPLEX Gold Genotyping Reagent Set</td>
			<td style="width:87px;">Sequenom</td>
			<td style="width:119px;">10158</td>
			<td>Reagents used for iPLEX assay including SAP kit.</td>
		</tr>
	</tbody>
</table>

a multi-detection assay for malaria transmitting mosquitoes

The Anopheles gambiae species complex includes the major malaria transmitting mosquitoes in Africa. Because these species are of such medical importance, several traits are typically characterized using molecular assays to aid in epidemiological studies. These traits include species identification, insecticide resistance, parasite infection status, and host preference. Since populations of the Anopheles gambiae complex are morphologically indistinguishable, a polymerase chain reaction (PCR) is traditionally used to identify species. Once the species is known, several downstream assays are routinely performed to elucidate further characteristics. For instance, mutations known as KDR in a para gene confer resistance against DDT and pyrethroid insecticides. Additionally, enzyme-linked immunosorbent assays (ELISAs) or Plasmodium parasite DNA detection PCR assays are used to detect parasites present in mosquito tissues. Lastly, a combination of PCR and restriction enzyme digests can be used to elucidate host preference (e.g., human vs. animal blood) by screening the mosquito bloodmeal for host-specific DNA. We have developed a multi-detection assay (MDA) that combines all of the aforementioned assays into a single multiplex reaction genotyping 33SNPs for 96 or 384 samples at a time. Because the MDA includes multiple markers for species, Plasmodium detection, and host blood identification, the likelihood of generating false positives or negatives is greatly reduced from previous assays that include only one marker per trait. This robust and simple assay can detect these key mosquito traits cost-effectively and in a fraction of the time of existing assays.

Species identification: 
The following 5 SNPs together identify three species (A. arabiensis, A. coluzzii and A. gambiae) (Table 4). If a sample is not one of the three species, the three SNPs (01073-213, 04679-157 and 10313-052) fail to amplify.
kdr genotype for inferring insecticide resistance: 
The 1014th codon of the para voltage-gated sodium channel cor...

Watch this Scientific Journal Video about A Multi-detection Assay for Malaria Transmitting Mosquitoes at JoVE.com

Wielowykrywalny test na komary przenoszące malarię | Biologia | Wideo

A Multi-detection Assay for Malaria Transmitting Mosquitoes

Malaria transmitting mosquitoes have a number of epidemiologically important characteristics that can only be detected using molecular techniques. Utilizing a MALDI-TOF based SNP genotyping platform, we developed an assay for simultaneously detecting multiple key traits (species, insecticide resistance, parasite infection and host choice) of malaria vectors.

The Anopheles gambiae species complex includes the major malaria transmitting mosquitoes in Africa. Because these species are of such medical importance, ...

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13.1K Views.  School of Veterinary Medicine, University of California - Davis. Malaria transmitting mosquitoes have a number of epidemiologically important characteristics that can only be detected using molecular techniques. Utilizing a MALDI-TOF based SNP genotyping platform, we developed an assay for simultaneously detecting multiple key traits (species, insecticide resistance, parasite infection and host choice) of malaria vectors.

Video: A Multi-detection Assay for Malaria Transmitting Mosquitoes

Injection of An. stephensi Embryos to Generate Malaria-resistant Mosquitoes

The introduction of exogenous genes into the genomes of mosquitoes requires microinjection techniques tailored to the specific species of interest. This video protocol demonstrates a method used by the James laboratory to microinject DNA constructs into Anopheles stephensi embryos for the generation of transformed mosquitoes. Techniques for preparing microinjection needles, collecting and preparing embryos and performing the microinjection are illustrated.

Anopheles stephensi mosquitoes are vectors for malaria inhabiting India and throughout Asia. This video demonstrates the technique for performing microinjections of this species with transgenes that will confer resistance to the malaria to the mosquito. Much of the methodology demonstrated in this video is applicable to microinjection techniques of other mosquito species.

The introduction of exogenous genes into the genomes of mosquitoes requires microinjection techniques tailored to the specific species of interest. This ...

Protocol for Dengue Infections in Mosquitoes (A. aegypti) and Infection Phenotype Determination

The purpose of this procedure is to infect the Aedes mosquito with dengue virus in a laboratory condition and examine the infection level and dynamic of the virus in the mosquito tissues. This protocol is routinely used for studying mosquito-virus interactions, especially for identification of novel host factors that are able to determine vector competence. The entire experiment must be conducted in a BSL2 laboratory. Similar to Plasmodium falciparum infections, proper attire including gloves and lab coat must be worn at all times. After the experiment, all the materials that came in contact with the virus need to be treated with 75% ethanol and bleached before proceeding with normal washing. All other materials need to be autoclaved before discarding them.

Protocol for Dengue Infections in Mosquitoes A. aegypti and Infection Phenotype Determination

Once a gene is identified as potentially refractory for the dengue virus, it must be evaluated for it's role in preventing viral infections within the mosquito. This protocol illustrates how the extent of dengue infections of mosquitoes can be assayed. The techniques for growing up the virus in culture, membrane feeding mosquitoes human blood, and assaying viral titers in the mosquito midgut are demonstrated.

The purpose of this procedure is to infect the Aedes mosquito with dengue virus in a laboratory condition and examine the infection level and dynamic of ...

Protocol for Mosquito Rearing (A. gambiae)

This protocol describes mosquito rearing in the insectary. The insectary rooms are maintained at 28&deg;C and ~80% humidity, with a 12 hr. day/night cycle. For this procedure, you'll need mosquito cages, 10% sterile sucrose solution, paper towels, beaker, whatman filter paper, glass feeders, human blood and serum, water bath, parafilm, distilled water, clean plastic trays, mosquito food (described below), mosquito net to cover the trays, vacuum, and a collection chamber to collect adults.

Protocol for Mosquito Rearing A. gambiae

This video illustrates the general techniques used to rear Anopheles gambiae in the laboratory. The methods for caring for laboratory mosquitoes are demonstrated through all stages of the organism's life cycle from larvae to pupae to blood-feeding adults.

This protocol describes mosquito rearing in the insectary. The insectary rooms are maintained at 28&deg;C and ~80% humidity, with a 12 hr. day/night ...

Protocol for Plasmodium falciparum Infections in Mosquitoes and Infection Phenotype Determination

Once a gene is identified as potentially refractory for malaria, it must be evaluated for its role in preventing Plasmodium infections within the mosquito.    This protocol illustrates how the extent of plasmodium infections of mosquitoes can be assayed.  The techniques for preparing the gametocyte culture, membrane feeding mosquitoes human blood, and assaying viral titers in the mosquito midgut are demonstrated.

Once a gene is identified as potentially refractory for malaria, it must be evaluated for its role in preventing Plasmodium infections within the mosquito. This protocol illustrates how the extent of plasmodium infections of mosquitoes can be assayed. The techniques for preparing the gametocyte culture, membrane feeding mosquitoes human blood, and assaying viral titers in the mosquito midgut are demonstrated.

Once a gene is identified as potentially refractory for malaria, it must be evaluated for its role in preventing Plasmodium infections within the ...

Population Replacement Strategies for Controlling Vector Populations and the Use of Wolbachia pipientis for Genetic Drive

In this video, Jason Rasgon discusses population replacement strategies to control vector-borne diseases such as malaria and dengue. "Population replacement" is the replacement of wild vector populations (that are competent to transmit pathogens) with those that are not competent to transmit pathogens. There are several theoretical strategies to accomplish this. One is to exploit the maternally-inherited symbiotic bacteria Wolbachia pipientis. Wolbachia is a widespread reproductive parasite that spreads in a selfish manner at the extent of its host's fitness. Jason Rasgon discusses, in detail, the basic biology of this bacterial symbiont and various ways to use it for control of vector-borne diseases.

In this interview, Jason Rasgon explains the concept of genetic drive and the characteristics of an effective gene drive system. The use of the endosymbiotic bacterium, Wolbachia pipientis, as a means to spread genes through mosquito populations, is hypothesized.

In this video, Jason Rasgon discusses population replacement strategies to control vector-borne diseases such as malaria and dengue. "Population ...

Protocol for RNAi Assays in Adult Mosquitoes (A. gambiae)

Reverse genetic approaches have proven extremely useful for determining  which genes underly resistance to vector pathogens in mosquitoes.  This video protocol illustrates a method used by the Dimopoulos lab to inject dsRNA into Anopheles gambiae mosquitoes, which harbor the malaria parasite.  The technique manipulating the injection setup and injecting dsRNA into the thorax is illustrated.

Protocol for RNAi Assays in Adult Mosquitoes A. gambiae

Reverse genetic approaches have proven extremely useful for determining which genes underly resistance to vector pathogens in mosquitoes. This video protocol illustrates a method used by the Dimopoulos lab to inject dsRNA into Anopheles gambiae mosquitoes, which harbor the malaria parasite. The technique manipulating the injection setup and injecting dsRNA into the thorax is illustrated.

Reverse genetic approaches have proven extremely useful for determining  which genes underly resistance to vector pathogens in mosquitoes.  This video ...

Preventing the Spread of Malaria and Dengue Fever Using Genetically Modified Mosquitoes

In this candid interview, Anthony A. James explains how mosquito genetics can be exploited to control malaria and dengue transmission.   Population replacement strategy, the idea that transgenic mosquitoes can be released into the wild to control disease transmission, is introduced, as well as the concept of genetic drive and the design criterion for an effective genetic drive system. The ethical considerations of releasing genetically-modified organisms into the wild are also discussed.

In this candid interview, Anthony A. James explains how mosquito genetics can be exploited to control malaria and dengue transmission. Population replacement strategy, the idea that transgenic mosquitoes can be released into the wild to control disease transmission, is introduced as well as the concept of genetic drive and the design criterion for an effective genetic drive system. The ethical considerations of releasing genetically-modified organisms into the wild are also discussed.

In this candid interview, Anthony A. James explains how mosquito genetics can be exploited to control malaria and dengue transmission.   Population ...

Building a Better Mosquito: Identifying the Genes Enabling Malaria and Dengue Fever Resistance in A. gambiae and A. aegypti Mosquitoes

In this interview, George Dimopoulos focuses on the physiological mechanisms used by mosquitoes to combat Plasmodium falciparum and dengue virus infections.   Explanation is given for how key refractory genes, those genes conferring resistance to vector pathogens, are identified in the mosquito and how this knowledge can be used to generate transgenic mosquitoes that are unable to carry the malaria parasite or dengue virus.

In this interview, George Dimopoulos focuses on the physiological mechanisms used by mosquitoes to combat Plasmodium falciparum and dengue virus infections. Explanation is given for how key refractory genes, those genes conferring resistance to vector pathogens, are identified in the mosquito and how this knowledge can be used to generate transgenic mosquitoes that are unable to carry the malaria parasite or dengue virus.

In this interview, George Dimopoulos focuses on the physiological mechanisms used by mosquitoes to combat Plasmodium falciparum and dengue virus ...

Transmitting Plant Viruses Using Whiteflies

Whiteflies, Hemiptera: Aleyrodidae, Bemisia tabaci, a complex of morphologically indistinquishable species5, are vectors of many plant viruses. Several genera of these whitefly-transmitted plant viruses (Begomovirus, Carlavirus, Crinivirus, Ipomovirus, Torradovirus) include several hundred species of emerging and economically significant pathogens of important food and fiber crops (reviewed by9,10,16). These viruses do not replicate in their vector but nevertheless are moved readily from plant to plant by the adult whitefly by various means (reviewed by2,6,7,9,10,11,17). For most of these viruses whitefly feeding is required for acquisition and inoculation, while for others only probing is required. Many of these viruses are unable or cannot be easily transmitted by other means. Therefore maintenance of virus cultures, biological and molecular characterization (identification of host range and symptoms)3,13, ecology2,12, require that the viruses be transmitted to experimental hosts using the whitefly vector. In addition the development of new approaches to management, such as evaluation of new chemicals14 or compounds15, new cultural approaches1,4,19, or the selection and development of resistant cultivars7,8,18, requires the use of whiteflies for virus transmission. The use of whitefly transmission of plant viruses for the selection and development of resistant cultivars in breeding programs is particularly challenging7. Effective selection and screening for resistance employs large numbers of plants and there is a need for 100% of the plants to be inoculated in order to find the few genotypes which possess resistance genes. These studies use very large numbers of viruliferous whiteflies, often several times per year.
Whitefly maintenance described here can generate hundreds or thousands of adult whiteflies on plants each week, year round, without the contamination of other plant viruses. Plants free of both whiteflies and virus must be produced to introduce into the whitefly colony each week. Whitefly cultures must be kept free of whitefly pathogens, parasites, and parasitoids that can reduce whitefly populations and/or reduce the transmission efficiency of the virus. Colonies produced in the manner described can be quickly scaled to increase or decrease population numbers as needed, and can be adjusted to accommodate the feeding preferences of the whitefly based on the plant host of the virus.
There are two basic types of whitefly colonies that can be maintained: a nonviruliferous and a viruliferous whitefly colony. The nonviruliferous colony is composed of whiteflies reared on virus-free plants and allows the weekly availability of whiteflies which can be used to transmit viruses from different cultures. The viruliferous whitefly colony, composed of whiteflies reared on virus-infected plants, allows weekly availability of whiteflies which have acquired the virus thus omitting one step in the virus transmission process.

Improving our understanding of and our ability to manage many of the insect-transmitted plant viruses requires the use of the vector. Insect transmission of plant viruses is a tritrophic interaction, and as such requires the manipulation of insects, virus, and plant. Vectors must be reared in large numbers and manipulated in such a way as to insure high rates of transmission to test plants. The basics of rearing and manipulating the whitefly, Bemisa tabaci (Hemiptera: Aleyrodidae), a vector of plant viruses belonging to several emerging plant virus genera, representing a large number of economically significant viruses is presented.

Whiteflies, Hemiptera: Aleyrodidae, Bemisia tabaci, a complex of morphologically indistinquishable species5, are vectors of many plant viruses. Several ...

Toxicological Assays for Testing Effects of an Epigenetic Drug on Development, Fecundity and Survivorship of Malaria Mosquitoes

Insecticidal resistance poses a major problem for malaria control programs. Mosquitoes adapt to a wide range of changes in the environment quickly, making malaria control an omnipresent problem in tropical countries. The emergence of insecticide resistant populations warrants the exploration of novel drug target pathways and compounds for vector mosquito control. Epigenetic drugs are well established in cancer research, however not much is known about their effects on insects. This study provides a simple protocol for examining the toxicological effects of 3-Deazaneplanocin A (DZNep), an experimental epigenetic drug for cancer therapy, on the malaria vector, Anopheles gambiae. A concentration-dependent increase in mortality and decrease in size was observed in immature mosquitoes exposed to DZNep, whereas the compound reduced the fecundity of adult mosquitoes relative to control treatments. In addition, there was a drug-dependent decrease in S-adenosylhomocysteine (SAH) hydrolase activity in mosquitoes following exposure to DZNep relative to control treatments. These protocols provide the researcher with a simple, step-by-step procedure to assess multiple toxicological endpoints for an experimental drug and, in turn, demonstrate a unique multi-prong approach for exploring the toxicological effects of water-soluble epigenetic drugs or compounds of interest against vector mosquitoes and other insects.

A protocol is developed to examine the effects of an epigenetic drug DZNep on the development, fecundity and survivorship of mosquitoes. Here we describe procedures for the aqueous exposure of DZNep to immature mosquitoes and a blood-based exposure of DZNep to adult mosquitoes in addition to measuring SAH hydrolase inhibition.

Insecticidal resistance poses a major problem for malaria control programs. Mosquitoes adapt to a wide range of changes in the environment quickly, making ...