We thank Ella Weinert, Michelle Helms and Marlis Badusche for excellent technical assistance, Jessica B&#246;rstler for analyses of Culex mosquitoes, Norbert Becker and Bj&#246;rn Pluskota for providing Aedes albopictus eggs and Olli Vapalahti for providing the virus stock. ML was supported by the Leibniz Association; grant number SAW-2014-SGN-3.

1. Prepare Female Mosquitoes
<ol>
	<li>Collect mosquitoes from a big cage by using an aspirator (approximately 400 mosquitoes per big cage).</li>
	<li>Anesthetize the mosquitoes with carbon dioxide (CO2) for 7 s.</li>
	<li>Sort 20 females per plastic vial (&#216; 50 mm &#215; 100 mm). 
	Note: If the mosquitoes wake up, use another 3 s of CO2.</li>
	<li>Starve the mosquitoes overnight.</li>
</ol>
2. Artificial Blood Meal
NOTE: All steps are performed under BSL-3 conditions.
<ol>
	<li>Prepare the infectious blood meal.
	<ol>
		<li>Dilute the virus stock to the concentration of 1 x 108 plaque forming units (PFU)/mL. 
		Note: The stock concentration was determined by performing Tissue culture infection dose 50 method (TCID50) and calculated by the Spearman &#38; K&#228;rber algorithm10,11.</li>
		<li>Mix expired human blood (blood preservation) from the blood bank (not suitable for human anymore, but useful for mosquitoes) with fructose (8% solution), filtrated bovine serum (FBS) and working solution of the virus stock (expired human blood:fructose:FBS:working solution = 5:3:1:1). 
		Note: We chose human blood, because this is the known natural mammal host of ZIKV.</li>
	</ol>
	</li>
	<li>Freeze 140 &#181;L of blood meal mix for further analysis via TCID50.</li>
	<li>Perform artificial feeding by using different feeding methods, depending on the species:
	<ol>
		<li>Aedes aegypti: Use a membrane feeding system for 30 min (1 mL per feeder).</li>
		<li>Culex spp.: Provide the infectious blood via a cotton stick overnight and do not warm up the blood (300 &#181;L per vial).</li>
		<li>Aedes albopictus: Put two droplets (50 &#181;L each) of the blood meal mix into the plastic vial and let the mosquitoes feed for 2 h. Do not warm up the blood. 
		Note: Mosquitoes will feed in the first 15 min. The prolonged incubation time is necessary due to safety reasons. The blood droplets are drained after 2 h, thus the contamination risk is reduced during the sorting of fed mosquitoes.</li>
	</ol>
	</li>
	<li>Anesthetize the mosquitoes with CO2 for 7 s. 
	NOTE: If the mosquitoes wake up, use another 3 s of CO2.</li>
	<li>Sort and count fully engorged mosquitoes into a new vial.</li>
	<li>Add a cotton pad, saturated with fructose (8% solution) between the vial and a plug.</li>
	<li>Keep the mosquitos at the designated temperature of 18 &#176;C or 27 &#176;C in the humidity of 80% for 14 or 21 days.</li>
	<li>Feed the mosquitos with fructose-saturated cotton pads. Replenish every 72 h with 1.5 mL of fructose (8% solution) per vial (up to 20 mosquitoes, depending on the feeding rate, see step 2.5).</li>
</ol>
3. Forced Salivation Assay on Day 14 or 21
NOTE: All steps are performed under BSL-3 conditions.
<ol>
	<li>Seed 2 x 104 Vero cells/per well in a 96 well plate with 200 &#181;L of growth medium (Dulbecco&#180;s modified eagle medium (DMEM) supplemented with 3% FBS, 100 U/mL penicillin, 100 mg/mL streptomycin, 5 &#181;g/mL amphotericin B, 2 mM L-glutamine, 1% non-essential amino acids (NEAA), 1% sodium pyruvate).</li>
	<li>Prepare the salivation device:
	<ol>
		<li>Place a squared glass plate (20 &#215; 20 cm) on the bench in an angle of 30&#176;. 
		Note: This is necessary due to the underpressure in the safety lab. If the plate is horizontal or vertical, liquid will leak.</li>
		<li>Place double sided adhesive tape on top of the glass plate.</li>
		<li>Role the modeling clay until it reaches a diameter of 0.5 cm and attach it horizontally 1 cm away from the double-sided adhesive tape.</li>
		<li>Cut off the first 0.3 cm of the tip of a 10 &#181;L filter tip. 
		NOTE: It is advised to prepare this before starting the experiment outside of the biosafety laboratory.</li>
		<li>Fill the filter tips with 10 &#181;L of phosphate buffered saline (PBS, pH 7.4).</li>
		<li>Place the filter tips on the modeling clay with the tip towards the sticky tape.</li>
		<li>Secure the filter tips with gentle pressure.</li>
	</ol>
	</li>
	<li>Prepare the mosquitoes:
	<ol>
		<li>Anesthetize the mosquitoes with CO2.</li>
		<li>Remove the legs and wings to immobilize the mosquitoes.</li>
		<li>Fix the living mosquito bodies on the sticky tape above a filter tip.</li>
		<li>Place the proboscis gently into the filter tip.</li>
		<li>Run the salivation assay for 30 min.</li>
		<li>Remove the filter tips and discard the clay and tape.</li>
	</ol>
	</li>
</ol>
4. Processing of Saliva
NOTE: Steps 4.1&#8211;4.6.2 are performed under BSL-3 conditions.
<ol>
	<li>Expel the contents into the reaction tubes containing 10 &#181;L of PBS.</li>
	<li>Mix gently and transfer the content into the wells of the prepared 96 well plate using one well per sample.</li>
	<li>Incubate the plate for 7 days at 37 &#176;C with 5% CO2.</li>
	<li>Use the binocular to check the cells for the presence of cytopathic effect (CPE).</li>
	<li>If the well is positive for CPE, harvest the supernatant by pipetting 140 &#181;L into a reaction tube for RNA extraction.</li>
	<li>Purify the RNA by using a RNA extraction kit.
	<ol>
		<li>Mix 140 &#181;L of the supernatant with 560 &#181;L of AVL buffer (viral lysis buffer) and incubate for 10 min at room temperature.</li>
		<li>Add 560 &#181;L of ethanol (96%) and vortex the sample. 
		NOTE: The samples are inactivated after this step and can be discharged out of the BSL-3 laboratory.</li>
		<li>Pipet 630 &#181;L of the sample onto a column and centrifuge with 6,000 x g for 1 min.</li>
		<li>Discard the filtrate, pipet the remaining 630 &#181;L on the column and repeat the centrifugation.</li>
		<li>Wash the RNA, bound to the membrane of the column, by adding 500 &#181;L of washing buffer 1 to the column and centrifuge at 6,000 x g for 1 min.</li>
		<li>Discard the collection tube and place the column into a new collection tube. Add 500 &#181;L washing buffer 2 and centrifuge at 12,500 x g for 3 min.</li>
		<li>Discard the collection tube and place the column into a 1.5 mL reaction tube.</li>
		<li>Add 50 &#181;L of elution buffer and incubate for 1 min at room temperature.</li>
		<li>Centrifuge at 6,000 x g for 1 min and then discard the column.</li>
	</ol>
	</li>
	<li>Analyze the samples for ZIKV RNA via RT-qPCR.</li>
</ol>
5. Processing of Mosquito Bodies
NOTE: Steps 5.1&#8211;5.5 are performed under BSL-3 conditions.
<ol>
	<li>Remove the bodies of the mosquito and place each body into a reaction tube. 
	NOTE: It is possible to pause the experiment at this point and store the samples at -80 &#176;C.</li>
	<li>Add 500 &#181;L of homogenization media (DMEM without any supplementals) into the reaction tube.</li>
	<li>Homogenize the body using hand motor mixer and use a new pistil for every sample.</li>
	<li>Add 200 &#181;L of the homogenate into a 96-well-plate for purification. 
	NOTE: It is possible to pause the experiment at this point and store the samples at -80 &#176;C.</li>
	<li>Inactivate the plate by incubation for 60 min at 60 &#176;C.</li>
	<li>Purify the RNA by automated nucleic acid purification. 
	NOTE: It is possible to pause the experiment at this point and store the samples at -80 &#176;C.</li>
</ol>
6. Analysis
<ol>
	<li>Quantify the Viral RNA Copies using RT-qPCR. 
	NOTE: The RNA copies were averaged over all ZIKV-positive mosquito bodies and without including the ZIKV-negative mosquitoes.</li>
	<li>Calculate the IR, defined as the number of ZIKV-positive mosquito bodies per number of fed females.</li>
	<li>Calculate the TR, defined as the number of mosquitoes with ZIKV-positive saliva per number of ZIKV-positive mosquito bodies. The transmission rate could not be calculated for species-temperature combinations with no ZIKV-positive bodies.</li>
</ol>

<ol>
	<li>Musso, D., Gubler, D. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Zika+Virus.">Zika Virus.</a> Clinical Microbiology Reviews. (3), 487-524 (2016).</li><li>Epelboin, Y., Talaga, S., Epelboin, L., Dusfour, I. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Zika+virus:+An+updated+review+of+competent+or+naturally+infected+mosquitoes.">Zika virus: An updated review of competent or naturally infected mosquitoes.</a> PLOS Neglected Tropical Diseases. 11 (11), e0005933 (2017).</li><li>Aliota, M. T., Peinado, S. A., Osorio, J. E., Bartholomay, L. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Culex+pipiens+and+Aedes+triseriatus+Mosquito+Susceptibility+to+Zika+Virus.">Culex pipiens and Aedes triseriatus Mosquito Susceptibility to Zika Virus.</a> Emerging Infectious Diseases. (10), 1857-1859 (2016).</li><li>Turell, M. J., Linthicum, K. J., Patrican, L. A., Davies, F. G., Kairo, A., Bailey, C. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vector+competence+of+selected+African+mosquito+(Diptera:+Culicidae)+species+for+Rift+Valley+fever+virus.">Vector competence of selected African mosquito (Diptera: Culicidae) species for Rift Valley fever virus.</a> Journal of Medical Entomology. 45 (1), 102-108 (2008).</li><li>Cornel, A. J., Jupp, P. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Comparison+of+three+methods+for+determining+transmission+rates+in+vector+competence+studies+with+Culex+univittatus+and+West+Nile+and+Sindbis+viruses.">Comparison of three methods for determining transmission rates in vector competence studies with Culex univittatus and West Nile and Sindbis viruses.</a> Journal of the American Mosquito Control Association. 5 (1), 70-72 (1989).</li><li>Hurlbut, H. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mosquito+salivation+and+virus+transmission.">Mosquito salivation and virus transmission.</a> The American Journal of Tropical Medicine and Hygiene. 15 (6), 989-993 (1966).</li><li>Anderson, S. L., Richards, S. L., Smartt, C. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+simple+method+for+determining+arbovirus+transmission+in+mosquitoes.">A simple method for determining arbovirus transmission in mosquitoes.</a> Journal of the American Mosquito Control Association. 26 (1), 108-111 (2010).</li><li>Heitmann, A., Jansen, S., L&#252;hken, R., Leggewie, M., Badusche, M., Pluskota, B., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Experimental+transmission+of+Zika+virus+by+mosquitoes+from+central+Europe.">Experimental transmission of Zika virus by mosquitoes from central Europe.</a> Eurovsurveillance. 22 (2), (2017).</li><li>Hierholzer, J. C., Killington, R. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Virus Isolation and Quantitation - Virology methods manual. , (1996).</li><li>Horzinek, R. W., Marian, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Kompendium+der+allgemeinen+Virologie.">Kompendium der allgemeinen Virologie.</a> Zentralblatt f&#252;r Veterin&#228;rmedizin R A. 32 (1-10), 480 (2010).</li><li>Richard, V., Paoaafaite, T., Cao-Lormeau, V. -. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vector+Competence+of+French+Polynesian+Aedes+aegypti+and+Aedes+polynesiensis+for+Zika+Virus.">Vector Competence of French Polynesian Aedes aegypti and Aedes polynesiensis for Zika Virus.</a> PLOS Neglected Tropical Diseases. 10 (9), (2016).</li><li>Fortuna, C., Remoli, M. E., Di Luca, M., Severini, F., Toma, L., Benedetti, E., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Experimental+studies+on+comparison+of+the+vector+competence+of+four+Italian+Culex+pipiens+populations+for+West+Nile+virus.">Experimental studies on comparison of the vector competence of four Italian Culex pipiens populations for West Nile virus.</a> Parasites &amp; Vectors. 8, 463 (2015).</li><li>Weger-Lucarelli, J., R&#252;ckert, C., Chotiwan, N., Nguyen, C., Garcia Luna, S. M., Turell, M. J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vector+Competence+of+American+Mosquitoes+for+Three+Strains+of+Zika+Virus.">Vector Competence of American Mosquitoes for Three Strains of Zika Virus.</a> PLOS Neglected Tropical Diseases. 10 (10), (2016).</li><li>Dubrulle, M., Mousson, L., Moutailler, S., Vazeille, M., Failloux, A. -. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Chikungunya+virus+and+Aedes+mosquitoes:+saliva+is+infectious+as+soon+as+two+days+after+oral+infection.">Chikungunya virus and Aedes mosquitoes: saliva is infectious as soon as two days after oral infection.</a> PLOS ONE. 4 (6), e5895 (2009).</li></ol>

The authors have nothing to disclose.

It has previously been shown that results obtained with forced salivation are in line with classical re-feeding experiments6. However, both in re-feeding experiments and in our presented method of forced salivation, it is impossible to directly proof salivation activity or monitor the release of saliva. To prove salivation activity, samples could be tested for other components present in the saliva (e.g., proteins, carbohydrates, etc.). Furthermore, additional qPCRs would allow detection of viral RNA copies. This, however, requires splitting of saliva samples for various analyses, which may limit sensitivity in the cell culture assay in case of very low particle numbers. In turn, this might lead to an underestimation of the determined transmission rates.
For reproducible results, it is necessary to ensure that all mosquitoes stay alive until the end of the experiment. This is controlled by visually monitoring the body movement activity of the mosquitoes. Furthermore, the principle use of the salivation assay for a given mosquito species has to be tested by feeding control viruses, which are known to be transmitted by this specific mosquito species. Vice versa, every virus introduced into an experiment has to be tested in a susceptible mosquito.
Forced salivation assays have many advantages. High numbers of mosquitoes can be tested simultaneously on a single specimen base under controlled standardized conditions without conflicting with animal welfare regulations9.
The method is used by several laboratories. However, exact setups may differ, which can lead to differences in results between laboratories. One critical component is the capillary to collect the saliva, which can be made of glass14 or plastic15. To comply with the high safety regulations of a biosafety level 3 insectary, we used plastic filter tips instead of glass capillaries, thus reducing the risk of injuries. Furthermore, filter tips have the advantage that the collected liquid can easily be transferred using a pipette.
The setup of the forced salivation assay presented here is based on two investigators working together and sharing duties. Demobilizing of the mosquito is performed by one person, while the other simultaneously prepares the forced salivation setup. This significantly reduces handling time and minimizes the risk of sample switching as changing between the demobilization-workplace and the salivation-plate is not necessary. Moreover, it allows placing the mosquitoes on the forced salivation device immediately after demobilization. This rather short mosquito handling time is essential for successful forced salivation. Lastly, the mosquitoes can be directly monitored for motility throughout the whole experiment.
The salivation assay presented here is used to gain insights into the vector potential of mosquito species. However, to answer some other specific questions (e.g., the numbers of mosquito bites that are needed to infect vertebrates), animal experiments might still be required.

In 2015, Zika virus (ZIKV), a mosquito-borne virus (mobovirus) belonging to the family Flaviviridae, emerged in Columbia and Brazil and spread rapidly across the Americas and the Caribbean, causing an epidemic with notable numbers of associated clinical cases of microcephaly and Guillain&#8211;Barr&#233; syndrome1. Mosquitoes of the species Aedes aegypti and Aedes albopictus are considered the primary and secondary vectors of ZIKV2, but other species of the genus Aedes have also proven to have experimental vector competence3. In contrast to Aedes species, most of the Culex species tested so far are not able to transmit the virus4. Merely, the data for Culex quinquefasciatus provided inconclusive results3. At present, information is lacking on mosquito vector competence for ZIKV under moderate temperature conditions (&#60;20 &#176;C). However, this information is substantial for the risk assessments of possible spreads to regions with temperate climate such as Central Europe.
A competent vector for ZIKV is able to acquire, maintain, amplify and finally transmit the virus. Therefore, testing the mosquito bodies or parts of the bodies, including legs, midgut, head or salivary glands, for ZIKV is not sufficient to determine vector competence. It is mandatory to test for infectious virus particles within released saliva. To assess vector competence, both infection rate (IR, number of ZIKV-positive mosquito bodies per number of engorged mosquitoes) and transmission rate (TR, number of mosquitoes with ZIKV-positive saliva per number of ZIKV-positive mosquito bodies), have to be determined. IRs of mosquitoes can be easily analyzed by simply homogenizing mosquitoes followed by a reverse-transcriptase real-time polymerase chain reaction (RT-qPCR) targeting ZIKV. Moreover, the infection can be further characterized by determining the viral copy numbers per mosquito. In contrast, the analysis of transmission rates relies on the detection of viable virus particles in the saliva of individual mosquitoes. This can be achieved by feeding of infected mosquitoes on susceptible host animals, followed by the analysis of the viremia in the host5. However, this method relies on suitable model organisms, and is costly and restricted by animal-welfare regulations. To avoid the use of laboratory animals for analyzing transmission rates and to reduce costs, artificial re-feeding systems using blood droplets have been described6. However, testing on individual scale combined with a high number of individuals is difficult and time-consuming. The first description of a salivation assay on individual scale was published in 19667 and during recent years, forced salivation experiments have become the method of choice to evaluate the vector competence of mosquitoes3,8.
Based on our vector competence study of Central European mosquitoes published recently9, we describe forced salivation as reported by Anderson et al.8 with some modifications. This method allows high throughput standardized experiments under high biosafety level conditions (BSL-3) and includes the identification of active virus by cell culture based assays. The experiments described here include 856 mosquitoes. They were infected with ZIKV by artificial blood meal and subsequently analyzed for the presence of infectious virus particles in the saliva. The mosquitoes introduced into the experiments comprised two long-established laboratory populations of Ae. aegypti and Culex pipiens pipiens biotype molestus (Cx. p. molestus), as well as field caught Culex pipiens pipiens biotype pipiens (Cx. p. pipiens), Culex torrentium (Cx. torrentium) and two Ae. albopictus populations. With the exception of one of the two Ae. albopictus populations, which was collected in Italy, all mosquitoes were collected in Germany.

<table>
	<tbody>
		<tr>
			<td>Inject+matic Sleeper</td>
			<td>Inject+matic</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Bugdorm-1 Insect Rearing Cage</td>
			<td>BugDorm Store</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Drosophila cultivation tubes</td>
			<td>carl roth</td>
			<td>PK11.2</td>
			<td>plastic vial for mosquitoes</td>
		</tr>
		<tr>
			<td>Plug for drosophila cultivation tubes</td>
			<td>carl roth</td>
			<td>PK15.1</td>
			<td></td>
		</tr>
		<tr>
			<td>Constant climate chamber</td>
			<td>Binder</td>
			<td>KBF-240</td>
			<td></td>
		</tr>
		<tr>
			<td>Blood</td>
			<td></td>
			<td></td>
			<td>banked human blood, expired, not usable for medical application</td>
		</tr>
		<tr>
			<td>Dumont-Pincette Electronic SS</td>
			<td>Dumont</td>
			<td>B40c</td>
			<td></td>
		</tr>
		<tr>
			<td>Vero cells</td>
			<td>BNITM</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Flash light aspirator</td>
			<td>Bioquip</td>
			<td>2809</td>
			<td></td>
		</tr>
		<tr>
			<td>double-sided adhesive tape</td>
			<td></td>
			<td></td>
			<td>no specific provider</td>
		</tr>
		<tr>
			<td>Gammex Powder-free gloves with AMT</td>
			<td>Ansell</td>
			<td></td>
			<td>for safety reasons necessary during work with pricks in the BSL3 laboratory</td>
		</tr>
		<tr>
			<td>RealStar Zika Virus RT-PCR-Kit</td>
			<td>altona diagnostics</td>
			<td>591013</td>
			<td></td>
		</tr>
		<tr>
			<td>MagMax Pathogen RNA/DNA Kit</td>
			<td>Thermo fisher scientific</td>
			<td>4462359</td>
			<td>RNA isolation of mosquito bodies</td>
		</tr>
		<tr>
			<td>Qiamp viral RNA Mini Kit</td>
			<td>Qiagen</td>
			<td>52906</td>
			<td>RNA-Isolation of supernatant</td>
		</tr>
		<tr>
			<td>filter tips (20 &#181;L)</td>
			<td>Sarstedt</td>
			<td>701,116,210</td>
			<td>Cut the first 3 mm of the tip</td>
		</tr>
		<tr>
			<td>hand motor mixer</td>
			<td>carl roth</td>
			<td>sold out</td>
			<td></td>
		</tr>
		<tr>
			<td>micro pestles for hand motor mixer</td>
			<td>carl roth</td>
			<td>CXH8.1</td>
			<td></td>
		</tr>
		<tr>
			<td>DMEM</td>
			<td></td>
			<td>P0403550</td>
			<td></td>
		</tr>
		<tr>
			<td>L Glutamine Penicilin/Streptomycin</td>
			<td>PAN</td>
			<td>P0819100</td>
			<td></td>
		</tr>
		<tr>
			<td>Amphotericin B</td>
			<td>PAN</td>
			<td>P06-0110</td>
			<td></td>
		</tr>
		<tr>
			<td>Fructose</td>
			<td>carl roth</td>
			<td>4981.5</td>
			<td></td>
		</tr>
		<tr>
			<td>Phosphate buffered saline</td>
			<td>PAN</td>
			<td>P04-36500</td>
			<td></td>
		</tr>
		<tr>
			<td>FBS</td>
			<td>PAN</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium Pyruvat</td>
			<td>PAN</td>
			<td>P0443100</td>
			<td></td>
		</tr>
		<tr>
			<td>MEM NAA</td>
			<td>PAN</td>
			<td>P0832100</td>
			<td></td>
		</tr>
		<tr>
			<td>Hemotek Feeder</td>
			<td>Hemotek</td>
			<td>PS6</td>
			<td></td>
		</tr>
		<tr>
			<td>Light Cycler</td>
			<td>Roche</td>
			<td>480 II</td>
			<td></td>
		</tr>
		<tr>
			<td>Light Cycler Software</td>
			<td>Roche</td>
			<td>480 SW 1.5.1</td>
			<td></td>
		</tr>
		<tr>
			<td>Modeling clay</td>
			<td></td>
			<td></td>
			<td>no specific provider</td>
		</tr>
		<tr>
			<td>King Fisher Flex Purification System</td>
			<td>ThermoFisher scientific</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Aedes albopictus</td>
			<td></td>
			<td></td>
			<td>eggs were collected in Freiburg, Germany</td>
		</tr>
		<tr>
			<td>Binocular</td>
			<td>MOTIC</td>
			<td>SMZ-168</td>
			<td></td>
		</tr>
		<tr>
			<td>Binocular light</td>
			<td>MOTIC</td>
			<td>MLC-150C</td>
			<td></td>
		</tr>
		<tr>
			<td>CO2-Incubator</td>
			<td>Thermo scientific</td>
			<td>MIDI 40</td>
			<td></td>
		</tr>
	</tbody>
</table>

forced salivation as a method to analyze vector competence of mosquitoes

Vector competence is defined as the potential of a mosquito species to transmit a mosquito-borne virus (mobovirus) to a vertebrate host. Viable virus particles are transmitted during a blood meal via the saliva of an infected mosquito. Forced salivation assays allow determining the vector potential on the basis of single mosquitoes, avoiding the use of animal experiments. The method is suitable to analyze a large number of mosquitoes in one experiment within a short period of time. Forced salivation assays were used to analyze 856 individual mosquitoes trapped in Germany, including two different Culex pipiens pipiens biotypes, Culex torrentium as well as Aedes albopictus, which were experimentally infected with Zika virus (ZIKV) and incubated at 18 &#176;C or 27 &#176;C for two and three weeks. The results indicated the lack of vector competence of the different Culex taxa for ZIKV. In contrast, Aedes albopictus was susceptible to ZIKV, but only at 27 &#176;C, with transmission rates similar to an Aedes aegypti laboratory colony tested in parallel.

Aedes aegypti is known as a competent vector for ZIKV at least under tropical climatic conditions12. Therefore, we used Ae. aegypti as a positive control to establish the assay and to analyze IRs as well as TRs at an incubation temperature of 27 &#176;C and a humidity of 80%. IR and TR were defined as previously described by Fortuna et al.13. Challenged Ae. aegypti showed IR of 50% and 72% and TR of 42% and 31% at 14 and 21 days post infection (dpi), respectively (Figure 1A and 1B). Subsequently, European mosquitoes were tested for ZIKV infection and transmission using tropical as well as temperate climatic conditions.
At 27 &#176;C incubation temperature, all mosquito species showed ZIKV infection at 14 dpi as well as 21 dpi, except Cx. p. pipiens and Cx. torrentium individuals, which were positive at 14 dpi only. All Aedes species showed higher IRs (between 50% and 72%) as well as higher viral RNA concentration (106 up to 109 RNA copies/mosquito specimens) in comparison to the different Culex taxa, which revealed IRs ranging between 0% and 32% and viral loads of 103 to 104 RNA copies/mosquito specimens. All Aedes species displayed ZIKV-positive saliva (TR 13&#8211;42%), whereas none of the saliva samples from the Culex taxa contained ZIKV (Figure 1A and 1B). Interestingly, transmission rates at 21 dpi were similar in Ae. aegypti and Ae. albopictus from Germany (30%), but were substantially lower in Ae. albopictus from Italy (13%).
Incubation of challenged mosquitoes at a moderate temperature of 18 &#176;C revealed generally lower virus loads in the Aedes species (104&#8211;106 RNA copies/mosquito) as well as in the different Culex taxa (102&#8211;104 RNA copies/mosquito). However, at 18 &#176;C incubation temperature, transmission of ZIKV was not observed for any of the mosquito species investigated.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/57980/57980fig1.jpg" /> 
Figure 1: Transmission rates of mosquitoes experimentally infected with ZIKV. Results of vector competence studies with ZIKV in different mosquito species. Six different mosquito taxa were infected with ZIKV and incubated at 27 &#176;C or 18 &#176;C for 14 (A) or 21 (B) days. TR is defined as the number of mosquitoes with ZIKV-positive saliva per number of ZIKV-positive mosquito bodies. The total number of mosquitoes investigated was 856, with a minimum of 30 individuals for each time point/temperature/mosquito taxa. <a href="https://www.jove.com/files/ftp_upload/57980/57980fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Forced Salivation As a Method to Analyze Vector Competence of Mosquitoes at JoVE.com

Forced Salivation As a Method to Analyze Vector Competence of Mosquitoes

For efficient control of mosquito borne virus transmission, the knowledge of the vector potential of respective mosquitoes is of particular interest. We describe forced salivation as a method to analyze vector competence of Aedes albopictus and three different Culex taxa for the transmission of Zika virus.

Vector competence is defined as the potential of a mosquito species to transmit a mosquito-borne virus (mobovirus) to a vertebrate host. Viable virus ...

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9.5K Views.  Bernhard Nocht Institute for Tropical Medicine. For efficient control of mosquito borne virus transmission, the knowledge of the vector potential of respective mosquitoes is of particular interest. We describe forced salivation as a method to analyze vector competence of Aedes albopictus and three different Culex taxa for the transmission of Zika virus.

Video: Forced Salivation As a Method to Analyze Vector Competence of 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 ...

Microinjection of A. aegypti Embryos to Obtain Transgenic Mosquitoes

In this video, Nijole Jasinskiene demonstrates the methodology employed to generate transgenic Aedes aegypti mosquitoes, which are vectors for dengue fever.  The techniques for correctly preparing microinjection needles, dessicating embryos, and performing microinjection are demonstrated.

In this video, Nijole Jasinskiene demonstrates the methodology employed to generate transgenic Aedes aegypti mosquitoes, which are vectors for dengue fever. The techniques for correctly preparing microinjection needles, dessicating embryos, and performing microinjection are demonstrated.

In this video, Nijole Jasinskiene demonstrates the methodology employed to generate transgenic Aedes aegypti mosquitoes, which are vectors for dengue ...

Use of Rotorod as a Method for the Qualitative Analysis of Walking in Rat

High speed videoanalysis of the details of movement can provide a source of information about qualitative aspects of walking movements. When walking on a rotorod, animals remain in approximately the same place making repetitive movements of stepping. Thus the task provides a rich source of information on the details of foot stepping movements. Subjects were hemi-Parkinson analogue rats, produced by injection of 6-hydroxydopamine (6-OHDA) into the right nigrostriatal bundle to deplete nigrostriatal dopamine (DA). The present report provides a video analysis illustration of animals previously were filmed from frontal, lateral, and posterior views as they walked (15). Rating scales and frame-by-frame replay of the video records of stepping behavior indicated that the hemi-Parkinson rats were chronically impaired in posture and limb use contralateral to the DA-depletion. The contralateral limbs participated less in initiating and sustaining propulsion than the ipsilateral limbs. These deficits secondary to unilateral DA-depletion show that the rotorod provides a use task for the analysis of stepping movements.

The rotorod test is used to assess motor status in the walking movement of hemi-Parkinson analogue rats.

High speed videoanalysis of the details of movement can provide a source of information about qualitative aspects of walking movements. When walking on a ...

Microinjection of Zebrafish Embryos to Analyze Gene Function

One of the advantages of studying zebrafish is the ease and speed of manipulating protein levels in the embryo.  Morpholinos, which are synthetic oligonucleotides with antisense complementarity to target RNAs, can be added to the embryo to reduce the expression of a particular gene product.  Conversely, processed mRNA can be added to the embryo to increase levels of a gene product.  The vehicle for adding either mRNA or morpholino to an embryo is microinjection.  Microinjection is efficient and rapid, allowing for the injection of hundreds of embryos per hour.  This video shows all the steps involved in microinjection.  Briefly, eggs are collected immediately after being laid and lined up against a microscope slide in a Petri dish.  Next, a fine-tipped needle loaded with injection material is connected to a microinjector and an air source, and the microinjector controls are adjusted to produce a desirable injection volume.  Finally, the needle is plunged into the embryo's yolk and the morpholino or mRNA is expelled.

This video shows how morpholino or mRNA can be injected into zebrafish embryos at the one-cell stage to decrease or increase the level of specific gene products during subsequent development.

One of the advantages of studying zebrafish is the ease and speed of manipulating protein levels in the embryo.  Morpholinos, which are synthetic ...

Lipid Vesicle-mediated Affinity Chromatography using Magnetic Activated Cell Sorting (LIMACS): a Novel Method to Analyze Protein-lipid Interaction

The analysis of lipid protein interaction is difficult because lipids are embedded in cell membranes and therefore, inaccessible to most purification procedures. As an alternative, lipids can be coated on flat surfaces as used for lipid ELISA and Plasmon resonance spectroscopy. However, surface coating lipids do not form microdomain structures, which may be important for the lipid binding properties. Further, these methods do not allow for the purification of larger amounts of proteins binding to their target lipids.
 To overcome these limitations of testing lipid protein interaction and to purify lipid binding proteins we developed a novel method termed lipid vesicle-mediated affinity chromatography using magnetic-activated cell sorting (LIMACS). In this method, lipid vesicles are prepared with the target lipid and phosphatidylserine as the anchor lipid for Annexin V MACS. Phosphatidylserine is a ubiquitous cell membrane phospholipid that shows high affinity to the protein Annexin V. Using magnetic beads conjugated to Annexin V the phosphatidylserine-containing lipid vesicles will bind to the magnetic beads. When the lipid vesicles are incubated with a cell lysate the protein binding to the target lipid will also be bound to the beads and can be co-purified using MACS. This method can also be used to test if recombinant proteins reconstitute a protein complex binding to the target lipid. 
 We have used this method to show the interaction of atypical PKC (aPKC) with the sphingolipid ceramide and to co-purify prostate apoptosis response 4 (PAR-4), a protein binding to ceramide-associated aPKC. We have also used this method for the reconstitution of a ceramide-associated complex of recombinant aPKC with the cell polarity-related proteins Par6 and Cdc42. Since lipid vesicles can be prepared with a variety of sphingo- or phospholipids, LIMACS offers a versatile test for lipid-protein interaction in a lipid environment that resembles closely that of the cell membrane. Additional lipid protein complexes can be identified using proteomics analysis of lipid binding protein co-purified with the lipid vesicles.

Lipid Vesicle-mediated Affinity Chromatography using Magnetic Activated Cell Sorting LIMACS: a Novel Method to Analyze Protein-lipid Interaction

To test the interaction of a protein with its target lipid we used MACS and Annexin V-conjugated magnetic beads and lipid vesicles synthesized from the target lipid and Annexin V-binding phosphatidylserine. Proteins bound to the target lipid are co-purified and analyzed after elution from the beads.

The analysis of lipid protein interaction is difficult because lipids are embedded in cell membranes and therefore, inaccessible to most purification ...

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.

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, ...

Maintaining Aedes aegypti Mosquitoes Infected with Wolbachia

Aedes aegypti mosquitoes experimentally infected with Wolbachia are being utilized in programs to control the spread of arboviruses such as dengue, chikungunya and Zika. Wolbachia-infected mosquitoes can be released into the field to either reduce population sizes through incompatible matings or to transform populations with mosquitoes that are refractory to virus transmission. For these strategies to succeed, the mosquitoes released into the field from the laboratory must be competitive with native mosquitoes. However, maintaining mosquitoes in the laboratory can result in inbreeding, genetic drift and laboratory adaptation which can reduce their fitness in the field and may confound the results of experiments. To test the suitability of different Wolbachia infections for deployment in the field, it is necessary to maintain mosquitoes in a controlled laboratory environment across multiple generations. We describe a simple protocol for maintaining Ae. aegypti mosquitoes in the laboratory, which is suitable for both Wolbachia-infected and wild-type mosquitoes. The methods minimize laboratory adaptation and implement outcrossing to increase the relevance of experiments to field mosquitoes. Additionally, colonies are maintained under optimal conditions to maximize their fitness for open field releases.

Maintaining Aedes aegypti Mosquitoes Infected with Wolbachia

Aedes aegypti mosquitoes infected with Wolbachia are being released into natural populations to suppress the transmission of arboviruses. We describe methods to rear Ae. aegypti with Wolbachia infections in the laboratory for experiments and field release, taking precautions to minimize laboratory adaptation and selection.

Aedes aegypti mosquitoes experimentally infected with Wolbachia are being utilized in programs to control the spread of arboviruses such as dengue, ...

Protocols for Testing the Toxicity of Novel Insecticidal Chemistries to Mosquitoes

New classes of insecticides with novel modes of action are needed to control insecticide resistant populations of mosquitoes that transmit diseases such as Zika, dengue and malaria. Assays for rapid, high-throughput analyses of unformulated novel chemistries against mosquito larvae and adults are presented. We describe protocols for single point-dose and dose response assays to evaluate the toxicity of small molecule chemistries to the Aedes aegypti vector of Zika, dengue and yellow fever,&#160;the malaria vector, Anopheles gambiae and the northern house mosquito, Culex quinquefasciatus, on contact and via ingestion. As an example, we evaluated the toxicity of amitriptyline, a small molecule antagonist of G protein-coupled receptors, via larval, adult topical and adult blood-feeding assay. The protocols provide a starting point to investigate insecticide potential. Results are discussed in the context of additional experiments to explore product applications and mechanisms for delivery.

Protocols are described for assessing the toxicity of chemistries to immature and adult mosquitoes for development as new classes of larvicides, adulticides and endectocides. The protocols enable high-throughput testing of multiple chemistries at single-point dose and subsequent evaluation via dose response assay to determine toxicity on contact or via ingestion.

New classes of insecticides with novel modes of action are needed to control insecticide resistant populations of mosquitoes that transmit diseases such ...

A Blood-Free Diet to Rear Anopheline Mosquitoes

Malaria research requires large-scale breeding and production conditions for mosquitoes (Anopheles spp.) in captivity. The sustainable and reliable production of mosquitoes is currently inhibited by the supply of fresh vertebrate blood. Alternatives to blood are required to promote efficient control strategies for malaria and other vector borne diseases that are transmitted by blood feeding insects. With this in mind, artificial liquid diets were formulated as substitutes for fresh vertebrate blood. Herein we report a blood-free artificial liquid diet that delivers feeding rates similar to blood and mimics the physiological effects of a fresh vertebrate blood meal. The diet induces ovarian and egg maturation of Anopheles mosquitoes and also produces good larval survival and development of functional adults. The formulated blood-free liquid diet is an important advance towards sustainable mosquito breeding in captivity and will reduce the maintenance costs of mosquito colonies and eliminate the need for fresh vertebrate blood.

A protocol is presented for formulation of a blood-free artificial diet to feed Anopheles mosquitoes in captivity. This diet has a similar performance to vertebrate blood and triggers oogenesis and egg maturation and produces viable adult progeny.

Malaria research requires large-scale breeding and production conditions for mosquitoes (Anopheles spp.) in captivity. The sustainable and reliable ...

Glomerular Outgrowth as an Ex Vivo Assay to Analyze Pathways Involved in Parietal Epithelial Cell Activation

Parietal epithelial cell (PEC) activation is one of the key factors involved in the development and progression of glomerulosclerosis. Inhibition of pathways involved in parietal epithelial cell activation could therefore be a tool to attenuate the progression of glomerular diseases. This article describes a method to culture and analyze parietal epithelial cell outgrowth of encapsulated glomeruli isolated from mouse kidney. After dissecting isolated mouse kidneys, the tissue is minced, and glomeruli are isolated by sieving. Encapsulated glomeruli are collected, and single glomeruli are cultured for 6 days to obtain glomerular outgrowth of parietal epithelial cells. During this period, parietal epithelial cell proliferation and migration can be analyzed by determining the cell number or the surface area of outgrowing cells. This assay can therefore be used as a tool to study the effects of an altered gene expression in transgenic- or knockout-mice or the effects of culture conditions on parietal epithelial cell growth characteristics and signaling. Using this method, important pathways involved in the process of parietal epithelial cell activation and consequently in glomerulosclerosis can be studied.

This article describes a method for culturing and analyzing glomerular parietal epithelial cell outgrowths of encapsulated glomeruli isolated from mouse kidney. This method can be used to study pathways involved in parietal epithelial cell proliferation and migration.

Parietal epithelial cell (PEC) activation is one of the key factors involved in the development and progression of glomerulosclerosis. Inhibition of ...

Forced Salivation As a Method to Analyze Vector Competence of Mosquitoes

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

Microinjection of A. aegypti Embryos to Obtain Transgenic Mosquitoes

Use of Rotorod as a Method for the Qualitative Analysis of Walking in Rat

Microinjection of Zebrafish Embryos to Analyze Gene Function

Lipid Vesicle-mediated Affinity Chromatography using Magnetic Activated Cell Sorting (LIMACS): a Novel Method to Analyze Protein-lipid Interaction

A Multi-detection Assay for Malaria Transmitting Mosquitoes

Maintaining Aedes aegypti Mosquitoes Infected with Wolbachia

Protocols for Testing the Toxicity of Novel Insecticidal Chemistries to Mosquitoes

A Blood-Free Diet to Rear Anopheline Mosquitoes

Glomerular Outgrowth as an Ex Vivo Assay to Analyze Pathways Involved in Parietal Epithelial Cell Activation