Name: Multiplexed Isothermal Amplification Based Diagnostic Platform to Detect Zika, Chikungunya, and Dengue 1 (Video) | JoVE Journal
Uploaded: 2018-03-13T13:30:00.000+00:00
Duration: 6 min 18 s
Description: Learn a multiplexed point-of-care diagnostic method for detecting Zika, chikungunya, and dengue viruses using isothermal amplification with minimal sample preparation. This technique enables rapid virus detection in resource-limited settings.

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The work was supported in part by FDOH-7ZK15 and NIAID 1R21AI128188-01. Research reported in this publication was supported in part by the National Institutes of Allergy and Infectious Diseases, and in part by Biomedical Research Program of Florida Department of Health. The content is solely the responsibility of the authors and does not necessarily represent the official views of the NIH or Florida Department of Health. Dynamic Combinatorial Chemistry LLC is acknowledged for their support and contribution to this project.
Dengue 1 virus (strain BOL-KW010) was kindly provided by the Florida Department of Health Bureau of Laboratories. Zika virus and the Asian lineage of chikungunya virus were graciously provided by the Centers for Disease Control and Prevention. The Indian Ocean lineage of chikungunya virus was kindly provided by Robert Tesh (World Reference Center for Emerging Viruses and Arboviruses, through the University of Texas Medical Branch in Galveston, Texas) to the UF-FMEL. We thank S. Bellamy, B. Eastmond, S. Ortiz, D. Velez, K. Wiggins, R. ZimLer, and K. Zirbel for assistance with the infection studies. We also thank M. S. Kim for providing Q-paper.

NOTE: Mosquitoes were the only animals directly used in this study. The procedures to manage chickens, whose blood was used to feed the infected mosquitoes, were approved as IACUC Protocol #201507682 by the University of Florida Institutional Animal Care and Use Committee.Virus propagation and mosquito infection studies were performed at the BSL-3 facility of the Florida Medical Entomology Laboratory in Vero Beach, FL. RT-LAMP experiments were performed in the BSL-2 laboratory shared by FfAME and Firebird Biomolecular Sciences LLC in Alachua, FL.
1. Design of Primers and Strand Displacing Probes
<ol>
	<li>Extract viral sequences for Dengue 1 from the Broad Institute database23; sequences for Zika and chikungunya from the NIAID Virus Pathogen Database and Analysis Resource24.
	<ol>
		<li>Create multiple sequence alignments (MSAs) for sequences of interest using software MUSCLE v3.8.3125. Use generated MSAs to search for LAMP primers sets within a conserved region of the target, and avoid non-relevant or unintended targets, such as distinctions between subtypes of a target.</li>
	</ol>
	</li>
	<li>Follow the design rules for LAMP primers as described online (http://loopamp.eiken.co.jp/e/lamp/), and allow the use of mixed bases in primers to cover the virus divergence26. To avoid cross-reactivity of primer sets, compare generated LAMP primers to the NCBI RNA virus database using NCBI BLAST27. Compare each set to eliminate primers that would dimerize in a multiplexed assay by using NCBI BLAST as well.</li>
	<li>Screen the double-stranded portion of the strand-displacing probe against any viral genome sequence and mosquito genomic sequence. Modify 5&#39;-ends of target binding probe with fluorescein amidite (FAM), HEX dye, and 5-carboxytetramethylrhodamine (TAMRA) dye for Zika, chikungunya, and Dengue 1, respectively.
	<ol>
		<li>Include a positive control primer set for urine samples. Design LAMP primers to target human mitochondrial DNA. Label strand-displacing probe with TET on 5&#39;-end. Label quencher probes that are partially complementary to each fluorescently labeled probe with quencher (e.g., Iowa Black-FQ) on 3&#39;-end (Table 1).</li>
	</ol>
	</li>
</ol>
2. Virus Isolates and Infected Mosquito Samples
<ol>
	<li>Use isolates of Zika virus (Puerto Rico strain), Chikungunya virus (La R&#233;union or British Virgin Islands strain), and Dengue serotype-1 virus (Key West strain). Determine viral titers using plaque assay28 or quantitative RT-PCR29. Extract viral RNAs using commercially available RNA extraction kits. 
	NOTE: Table 2 represents the viral titers of each virus isolate used in this study.</li>
	<li>Follow the article published by Yaren et al. for a detailed protocol about the infection of Ae. aegypti females with Zika and chikungunya viruses20. See Table 2 for the viral titer of the mosquito sample infected with Zika virus.</li>
</ol>
3. RT-LAMP Coupled with Thermolabile Uracil DNA Glycosylase
<ol>
	<li>10X primer mix preparation.
	<ol>
		<li>Prepare 100 &#181;M stock solution of each primer and probe (see step 1) by adding nuclease free water. Vortex well and store at -20 &#176;C until use.</li>
		<li>For 10X Primer mix for each Zika, Dengue 1, or mitochondrial DNA target, mix 16 &#181;L of FIP, 16 &#181;L BIP, 2 &#181;L of F3, 2 &#181;L of B3, 5 &#181;L of LF, 2 &#181;L of LB, 3 &#181;L of LB-fluorescent labeled probe, 4 &#181;L of quencher probe, and 50 &#181;L of nuclease-free water to give a total of 100 &#181;L volume.</li>
		<li>For 10X Primer mix for Chikungunya, mix 16 &#181;L of FIP, 16 &#181;L BIP, 2 &#181;L of F3, 2 &#181;L of B3, 5 &#181;L of LB, 2 &#181;L of LF, 3 &#181;L of LF-fluorescent labeled probe, 4 &#181;L of quencher probe, and 50 &#181;L of nuclease-free water to give a total of 100 &#181;L volume. 
		NOTE: The probe concentration described above uses 300 nM of final fluorescent probe and 400 nM of quencher probe. Alternatively, use 80 nM of fluorescently labeled probe and 200 nM of its quencher probe for real-time analysis.</li>
	</ol>
	</li>
	<li>Add 5 &#181;L of 10X primer mix (For 3-plex, add 5 &#181;L of each 10X primer mix), 5 &#181;L of 10X isothermal amplification buffer (1X buffer composition: 20 mM Tris-HCl buffer pH 8.8, 50 mM KCl, 10 mM (NH4)2SO4, 8 mM MgSO4, 0.1% Tween-20, 1 mM DTT), 7 &#181;L of dNTP mixture (10 mM of dATP, dCTP and dGTP; 5 mM of dTTP and dUTP), 16 units of DNA Polymerase, 15 units of Reverse Transcriptase, 80 units of recombinant ribonuclease inhibitor, 2 units of thermolabile UDG, 1-2 &#181;L of varying amounts of viral RNAs, and water to bring the total volume up to 50 &#181;L in a 0.25 mL PCR tube (see Table of Materials).</li>
	<li>Include negative control assays at this stage by replacing viral RNA volume with water. Incubate samples between 65-68 &#176;C for 45 min to 1 h, then analyze by running 5 &#181;L of each sample on 2.5% agarose gel in 1X TBE buffer containing ethidium bromide (0.4 &#181;g/mL). Use a 25 bp or 50 bp DNA ladder as marker on the gel. 
	NOTE: Addition of a non-target specific template is optional.</li>
	<li>To detect the presence of pathogenic RNA, test each primer set and its no-template control by varying the temperature and/or magnesium concentration, since each RT-LAMP primer set was designed to work in varying temperatures (65 &#176;C to 68 &#176;C) or magnesium concentrations (6 to 10 mM final). Prepare the experiments at room temperature.</li>
</ol>
4. RT-LAMP Using Viral RNA-Spiked Urine
<ol>
	<li>Test RT-LAMP primers in varying final concentrations of urine (0%, 10%, 20%, and 50%) in 50 &#181;L of total reaction volume. For 10% final urine concentration, add 1 &#181;L of viral RNA to 5 &#181;L of urine. For 20% final urine concentration, add 1 &#181;L of viral RNA to 10 &#181;L of urine. For 50% final urine concentration, add 1 &#181;L of viral RNA to 25 &#181;L of urine.</li>
	<li>For real-time monitoring of RT-LAMP in 10% of urine, use a real-time PCR instrument (see Table of Materials) with different fluorophore filters.
	<ol>
		<li>To read fluorescence signals from FAM-labeled amplicons for Zika, use a filter ranging from 483 to 533 nm; for HEX-labeled amplicons for chikungunya, use a filter ranging from 523 to 568 nm; for TAMRA-labeled amplicons for Dengue 1, use a filter ranging from 558 to 610 nm; and for TET-labeled amplicons for mitochondrial DNA, use a filter ranging from 523 to 568 nm. 
		NOTE: FAM has excitation and emission maxima of 495 nm and 520 nm, respectively. HEX has excitation and emission maxima of 538 nm and 555 nm, respectively. TAMRA has excitation and emission maxima of 559 nm and 583 nm, respectively. TET has excitation and emission maxima of 522 nm and 539 nm, respectively.</li>
	</ol>
	</li>
	<li>Use 96-well plates and seal the plate with a clear plastic sheet, then incubate samples at 65-68 &#176;C for 60-90 min and record the fluorescence every 30 s using the light cycler. Initially use 80 nM of fluorescently labeled probes, and then test the 300 nM of fluorescently labeled probes.
	<ol>
		<li>Determine limit of detection for each target by adding serially diluted viral RNAs in final urine concentration of 10%. 
		NOTE: Use real-time RT-LAMP to determine optimum temperature, magnesium concentration, fluorescently labeled probe concentration, and reaction time.</li>
	</ol>
	</li>
	<li>To visualize the fluorescence generated by strand displaceable probes by eye, use a blue LED light source from a light cycler with excitation at 470 nm (any gel electrophoresis box with built-in blue light source will work, see table of materials), and record the image with a cell phone camera at room temperature in the dark. 
	NOTE: Use 300 nM of fluorescently labeled probes, when visualization of all three colors by eye using blue LED is needed.</li>
</ol>
5. RT-LAMP on Detection of Zika-Infected Mosquitoes Using Q-Paper Technology
<ol>
	<li>Prepare quaternary ammonium-modified filter paper (Q-paper), according to previously published methods with slight modifications30.
	<ol>
		<li>Immerse 1 g of cellulose filter paper circles (see Table of Materials) with diameters of 3.5 cm in 50 mL of 1.8% of aqueous NaOH solution for 15 min for activation.</li>
		<li>Collect activated paper circles by vacuum filtration and then immerse them in 40 mL of aqueous solution of (2,3-epoxypropyl) trimethylammonium chloride (0.28 g) overnight at room temperature. 
		NOTE: Keep the mass ratio of (2,3-epoxypropyl) trimethylammonium chloride to filter paper at 0.28 to 1.</li>
		<li>Collect the resulting cationic paper by vacuum filtration, and neutralize with 50 mL of 1% of acetic acid.</li>
		<li>Wash the paper three times with ethanol and air-dry under a hood with constant airflow.</li>
	</ol>
	</li>
	<li>Cut Q-paper sheets into small rectangles (3 mm x 4 mm) using a paper punch or scissors. Crush Ae. aegypti female mosquitoes potentially infected with Zika on each paper with a micro pestle.</li>
	<li>Add to each paper 20 &#181;L of 1 M aqueous ammonia solution (pH &#8776; 12) and wait for 5 min. Then wash each paper once with 20 &#181;L of 50% EtOH and once with 20 &#181;L of nuclease-free water. Air-dry the paper in BSL-2 biosafety cabinet for about 1 h. 
	NOTE: At this point, samples can be stored at -20 &#176;C overnight until use.</li>
	<li>Using tweezers, place each paper in 100 &#181;L of RT-LAMP reaction mixture and incubate at 65-68 &#176;C for 45 min. Make sure to fully submerge the paper in the solution; it should not be floating. Read and record the fluorescence arising from Zika virus using blue LED light source and orange or yellow filter.</li>
</ol>
6. Lyophilization of RT-LAMP Reagents for 100 &#181;L of Reaction Volume
<ol>
	<li>Prepare 10X LAMP primer mixture according to section 3.1, and prepare dNTP mixture containing dUTP according to section 3.2. Store primer mixture and dNTPs at -20 &#176;C until use.</li>
	<li>Prepare 10 mL of enzyme dialysis buffer to remove glycerol, by mixing 100 &#181;L of 1 M Tris-HCl pH 7.5, 500 &#181;L of 1 M KCl, 2 &#181;L of 0.5 M EDTA, 100 &#181;L of 10% Triton X-100, 100 &#181;L of 0.1 M DTT and 9.198 mL of nuclease-free water. Store the dialysis buffer at 4 &#176;C. 
	NOTE: Make sure to filter (0.2-micron filters) all buffer reagent solutions prior to use and store them at 4 &#176;C.
	<ol>
		<li>Use an ultrafiltration membrane with 10 kDa cut-off limit (see Table of Materials). Place 350 &#181;L of dialysis buffer, 4 &#181;L of 32 units of DNA Polymerase, 2 &#181;L of 30 units of Reverse Transcriptase, and 2 &#181;L of 80 units of RNase inhibitor into ultrafiltration membrane and centrifuge at 14,000 x g for 5 min at 4 &#176;C.</li>
		<li>Add another 350 &#181;L of dialysis buffer to the ultrafiltration membrane and centrifuge (14,000 x g) for another 5 min. Empty the collection tube and repeat this step, then centrifuge (14,000 x g) for 3 min.</li>
		<li>For elution, invert the membrane and place in a new collection tube. Spin at 1,000 x g for 2 min. Measure the elution volume; if less than 8 &#181;L, bring the volume up to 8 &#181;L by adding dialysis buffer. Store the elution at 4 &#176;C, and immediately proceed to next step. 
		NOTE: This protocol is for single tube lyophilization, but prepare at least 10 reaction tubes at a time using the same ultrafiltration membrane and use the same amount of dialysis buffer.</li>
	</ol>
	</li>
	<li>Mix 10 &#181;L of 10X LAMP primer if singleplex (for 3-plex, add 10 &#181;L of each 10X primer mix), 14 &#181;L of dNTP mixture, 8 &#181;L of dialyzed enzyme mix, 2 &#181;L of 2 units of thermolabile UDG, and 66 &#181;L of nuclease free water (for 3-plex, use 46 &#181;L) in a 0.5 mL microcentrifuge tube and leave the lid open. Instead, add another lid punctured with a needle to allow vapor to escape.</li>
	<li>Immediately freeze the tubes at -80 &#176;C for 2 h, and lyophilize the tube for 4 h. Cover the lyophilization chamber with aluminum foil for protection from light. When reagents are dried, remove the punctured lids, close the original lid, and store the tubes with lyophilized reagents at 4 &#176;C in the dark. 
	NOTE: Reagents can be lyophilized overnight, if necessary.</li>
</ol>
7. Testing Lyophilized RT-LAMP Reagents on Urine and Mosquito Samples Containing Zika
<ol>
	<li>Use the following items from the kit (see the Table of Materials) for Zika: A 3D-printed observing box with orange filter (long pass filter, cut-on ~540 nm), 2 AAA batteries for observing box, lyophilized reaction tubes labeled ZV for Zika detection, and 1.1X rehydration Buffer in 1.5 mL screw top tubes.</li>
	<li>Prepare 50 mL of 1.1X rehydration buffer by mixing 5.5 mL of 10X isothermal amplification buffer that comes along with DNA Polymerase (see the Table of Materials), 3.3 mL of 100 mM MgSO4, 110 &#181;L of 0.5 M DTT, and 41.09 mL of nuclease-free water. Mix well, aliquot 1 mL of this solution to 1.5 mL screw top tubes, and store at 4 &#176;C until use.</li>
	<li>Add 90 &#181;L of 1.1X rehydration buffer to each reaction tube (0.5 mL). Ensure that the liquid fills the bottom of the tube containing the lyophilized reagents (dissolve them with mixing by shaking, then briefly spin down (1,000 x g)). Add 10 &#181;L of urine sample spiked with viral RNA to the reaction tubes (see section 4.1 for details).
	<ol>
		<li>If testing mosquitoes, add a rectangle of Q-paper holding mosquito carcasses (as prepared in the steps described in sections 5.2 and 5.3), along with 10 &#181;L purified water instead of urine samples. 
		NOTE: Alternatively, add 10 &#181;L of saliva or serum samples instead of urine. If the samples are extracted DNA or RNA, add 2-5 &#181;L of the sample into rehydrated mixture and complete with nuclease-free water to 10 &#181;L of final sample volume.</li>
	</ol>
	</li>
	<li>Close the lid of the reaction tubes. Place them in a heat block/bath (or incubator) pre-set at 65-68 &#176;C. Incubate for 30-45 min, but no more than 1 h. After incubation, remove the tube from the heat. To prevent contamination of future assays, ensure that these tubes remain closed.</li>
	<li>Place reaction tubes in the observing box; the temperature will fall to the ambient temperature (preferably 25 &#176;C). Turn on the switch on the back of the observing box. Observe sample through the orange filter and capture the image by a cell phone camera which is held at a distance where the image fills 80% of the field of view. 
	NOTE: Better visualization is achieved in low light environments.</li>
	<li>After visualization is completed, turn off the switch. Store the sealed tubes in the dark, preferably with refrigeration, if later visualization is needed.</li>
</ol>

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<li>Edgar, R. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((MUSCLE%3A+multiple+sequence+alignment+with+high+accuracy+and+high+throughput%5BTitle%5D)+AND+%22Nucleic+Acids+Res%22%5BJournal%5D)">MUSCLE: multiple sequence alignment with high accuracy and high throughput.</a> Nucleic Acids Res. 32, (2004).</li>
<li>Boonham, N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Methods+in+virus+diagnostics%3A+from+ELISA+to+next+generation+sequencing%5BTitle%5D)+AND+%22Virus+Res%22%5BJournal%5D)">Methods in virus diagnostics: from ELISA to next generation sequencing.</a> Virus Res. 186, (2014).</li>
<li>Altschul, S. F., Gish, W., Miller, W., Myers, E. W., Lipman, D. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Basic+local+alignment+search+tool%5BTitle%5D)+AND+%22J+Mol+Biol%22%5BJournal%5D)">Basic local alignment search tool.</a> J Mol Biol. 215, (1990).</li>
<li>Baer, A., Kehn-Hall, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Viral+Concentration+Determination+Through+Plaque+Assays%3A+Using+Traditional+and+Novel+Overlay+Systems%5BTitle%5D)+AND+%22Journal+of+visualized+experiments%3A+JoVE%22%5BJournal%5D)">Viral Concentration Determination Through Plaque Assays: Using Traditional and Novel Overlay Systems.</a> Journal of visualized experiments: JoVE. (93), e52065(2014).</li>
<li>Reiskind, M. H., Pesko, K., Westbrook, C. J., Mores, C. N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Susceptibility+of+Florida+Mosquitoes+to+Infection+with+Chikungunya+Virus%5BTitle%5D)+AND+%22The+American+journal+of+tropical+medicine+and+hygiene%22%5BJournal%5D)">Susceptibility of Florida Mosquitoes to Infection with Chikungunya Virus.</a> The American journal of tropical medicine and hygiene. 78 (3), 422-425 (2008).</li>
<li>Glushakova, L. G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Detection+of+chikungunya+viral+RNA+in+mosquito+bodies+on+cationic+%28Q%29+paper+based+on+innovations+in+synthetic+biology%5BTitle%5D)+AND+%22Journal+of+Virological+Methods%22%5BJournal%5D)">Detection of chikungunya viral RNA in mosquito bodies on cationic (Q) paper based on innovations in synthetic biology.</a> Journal of Virological Methods. 246, 104-111 (2017).</li>
<li>Hsieh, K., Mage, P. L., Csordas, A. T., Eisenstein, M., Tom Soh, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Simultaneous+elimination+of+carryover+contamination+and+detection+of+DNA+with+uracil-DNA-glycosylase-supplemented+loop-mediated+isothermal+amplification+%28UDG-LAMP%29%5BTitle%5D)+AND+%22Chemical+Communications%22%5BJournal%5D)">Simultaneous elimination of carryover contamination and detection of DNA with uracil-DNA-glycosylase-supplemented loop-mediated isothermal amplification (UDG-LAMP).</a> Chemical Communications. 50 (28), 3747-3749 (2014).</li>
<li>Tang, Y., Chen, H., Diao, Y. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Advanced+uracil+DNA+glycosylase-supplemented+real-time+reverse+transcription+loop-mediated+isothermal+amplification+%28UDG-rRT-LAMP%29+method+for+universal+and+specific+detection+of+Tembusu+virus%5BTitle%5D)+AND+%22Sci+Rep%22%5BJournal%5D)">Advanced uracil DNA glycosylase-supplemented real-time reverse transcription loop-mediated isothermal amplification (UDG-rRT-LAMP) method for universal and specific detection of Tembusu virus.</a> Sci Rep. 6, 27605(2016).</li>
<li>Thomas, A. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Fluorescence+of+pterin%2C+6-formylpterin%2C+6-carboxypterin+and+folic+acid+in+aqueous+solution%3A+pH+effects%5BTitle%5D)+AND+%22Photochem+Photobiol+Sci%22%5BJournal%5D)">Fluorescence of pterin, 6-formylpterin, 6-carboxypterin and folic acid in aqueous solution: pH effects.</a> Photochem Photobiol Sci. 1, (2002).</li>
<li>Wu, D., Lehane, M. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Pteridine+fluorescence+for+age+determination+of+anopheles+mosquitoes%5BTitle%5D)+AND+%22Med+Vet+Entomol%22%5BJournal%5D)">Pteridine fluorescence for age determination of anopheles mosquitoes.</a> Med Vet Entomol. 13, (1999).</li>
<li>Janis, A. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Inactivation+and+environmental+stability+of+Zika+virus%5BTitle%5D)+AND+%22Emerg+Infect+Dis+J%22%5BJournal%5D)">Inactivation and environmental stability of Zika virus.</a> Emerg Infect Dis J. 22, (2016).</li>
<li>Poloni, T. R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Detection+of+dengue+virus+in+saliva+and+urine+by+real+time+RT-PCR%5BTitle%5D)+AND+%22Virology+Journal%22%5BJournal%5D)">Detection of dengue virus in saliva and urine by real time RT-PCR.</a> Virology Journal. 7 (1), 22(2010).</li>
<li>Jones, P., Okeoma, C. <a target="_blank" href="https://www.omicsonline.org/open-access/detection-of-chikungunya-virus-chikv-in-urine-of-infected-mice-a-potential-noninvasive-diagnostic-tool-for-chikv-2332-0877-1000226.php?aid=59212">Detection of Chikungunya virus (CHIKV) in urine of infected mice: a potential non-invasive diagnostic tool for CHIKV.</a> J Infect Dis Ther. 3 (4), 1000226(2015).</li>
<li>Glushakova, L. G., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((High-throughput+multiplexed+xMAP+Luminex+array+panel+for+detection+of+twenty+two+medically+important+mosquito-borne+arboviruses+based+on+innovations+in+synthetic+biology%5BTitle%5D)+AND+%22J.+Virol.+Methods%22%5BJournal%5D)">High-throughput multiplexed xMAP Luminex array panel for detection of twenty two medically important mosquito-borne arboviruses based on innovations in synthetic biology.</a> J. Virol. Methods. 214, 60-74 (2015).</li>
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</ol>

Several of the authors and their institutions own intellectual property associated with this assay.

Mosquito-borne viruses including Zika, chikungunya, and dengue threaten the public health and recent Zika outbreaks highlight the need for low-cost point-of-care detection alternatives for patient diagnostics, as well as for mosquito surveillance. Isothermal amplification methods were developed as affordable alternatives to PCR-based systems. Particularly, RT-LAMP-based platforms have been applied to detect a wide range of pathogens. However, the use of isothermal platforms has been mainly limited to single target detect...

Mosquito-borne virus infections, including dengue, chikungunya, and Zika viruses are on the rise and demand immediate management strategies. Dengue and chikungunya viruses are already endemic in many of the tropical regions where Zika is now spreading in the Western Hemisphere1. Zika virus, like dengue, is a member of the Flaviviridae family and is native to Africa with one Asian and two African genetic lineages2. Even though the identification of the Zika virus dates back to 1947, Zika infection in humans remained sporadic for a half century before emerging in the Pacific and the Americas. The first reported outbreak of Zika fever occurred on the island of Yap in the Federated States of Micronesia in 2007, followed by French Polynesia in 2013 and 2014. The first major outbreak in the Americas occurred in 2015 in Brazil.
Zika, chikungunya, and dengue viruses are primarily transmitted by Aedes aegypti and Aedes albopictus. However, Zika has additional downstream human-to-human transmission possibilities, likely being spread through sexual contact, mother-to-fetus interaction, and via breast-feeding3,4,5. Zika fever was first believed to cause only mild illness. However, it was later associated with Guillain-Barr&#233; syndrome in adults, microcephaly in neonates, and chronic musculoskeletal diseases that may last months to years. Diagnosis of Zika illness can be challenging, since the symptoms of a Zika infection are similar to those of other mosquito-spread viruses6. Common co-infections of these viruses make differential diagnosis even more challenging7,8. Therefore, rapid and reliable detection of the nucleic acids from Zika and other viruses is needed to understand epidemiology in real time, to initiate control and preventive measures, and to manage patient care9.
Current diagnostic tests for these viruses include serological tests, virus isolation, virus sequencing, and reverse-transcription PCR (RT-PCR). Standard serological approaches often suffer from inadequate sensitivity and results can be complicated by cross-reactivity in patients who have previously been infected by other flaviviruses.
Therefore, nucleic acid testing remains the most reliable way to detect and differentiate these viruses. Detection of Zika and other mosquito-borne viruses is usually performed using RT-PCR or real-time RT-PCR in variety of biological fluids, such as serum, urine, saliva, semen, breast milk, and cerebral fluid10,11. Urine and saliva samples are generally preferred over blood, since they exhibit less PCR-inhibition, higher viral loads, virus presence for longer periods of time, and increased ease of collection and handling12,13. RT-PCR-based diagnostic tests, however, comprise extensive sample preparation steps and expensive thermal cycling equipment, making it less optimal for the point-of-care.
Reverse transcription loop-mediated isothermal amplification (RT-LAMP) has emerged as a powerful RT-PCR alternative due to its high sensitivity and specificity14, its tolerance for inhibitory substances in biological samples15, and operation on single temperature, which significantly lowers assay complexity and associated costs, making it suitable for low resource environments. RT-LAMP, as it is classically implemented, comprises six primers that bind to eight distinct regions within the target RNA. It runs at constant temperatures between 60 &#176;C and 70 &#176;C, and uses a reverse transcriptase and a DNA polymerase with strong strand displacing activity.
During the initial stages of RT-LAMP, forward and backward internal primers (FIP and BIP, Figure 1A) along with outer forward and backward primers (F3 and B3) form a dumbbell structure, the seed structure of exponential LAMP amplification. Amplification is further accelerated by the loop forward and backward primers (LF and LB), which are designed to bind the single stranded regions of the dumbbell, and results in the formation of concatemers with multiple repeating loops16. Classical LAMP assays based on turbidity or readout by DNA intercalating dyes is not entirely suited for point-of-care detection of Zika, where some level of multiplexing is desired17,18,19. Multiplexing is not easily obtained in these systems, as they are prone to generate false-positives due to off-target amplifications.
To manage these issues, the literature adds an additional component in the form of a &#34;strand-displacing probe&#34; to the classical RT-LAMP architecture20,21,22. Each probe has a sequence-specific double-strand region and a single-stranded priming region. The probe with the single-stranded region is tagged with a 5&#39;-fluorophore, and the complementary probe is modified with a 3&#39;-end quencher. In the absence of a target, no fluorescence is observed due to hybridization of the complementary probe strands, which brings the fluorophore and quencher into close proximity. In the presence of a target, the single-stranded portion of the fluorescent probe binds to its complement on the target, and is then extended by a strand displacing polymerase. Further polymerase extension by reverse primers causes the separation of the quencher strand from its complementary fluorescently labeled strand, allowing emission of fluorescence (Figure 1B). With this design, the signal is generated after the dumbbell formation, reducing the chances of false-positive signals.
The double-stranded portion of the strand-displacing probe can be any sequence, and when multiplexing is applied, the same sequence may be used with different fluorophore-quencher pairs. With this architecture, virus-contaminated urine, serum, or mosquito samples squished on paper were directly introduced to the assay without sample preparation. Three-color fluorescence read-outs visible to human eye were generated within 30 - 45 min, and signals were visualized by a 3D-printed observation box that uses a blue LED and an orange filter. Freeze-drying the RT-LAMP reagents enabled deployment of this kit to lower resource settings without a need for refrigeration.

<table><tbody><tr><td>SafeBlue Illuminator/ Electrophoresis System, MBE-150-PLUS</td><td>Major Science</td><td>MBE-150</td><td>Gel electrophoresis</td></tr><tr><td>G:BOX F3</td><td>Syngene</td><td>G:BOX F3</td><td>Gel imaging</td></tr><tr><td>LightCycler 480 Instrument II, 96-well</td><td>Roche Applied Science</td><td>05 015 278 001</td><td>Real-time PCR</td></tr><tr><td>Amicon Ultra-0.5 Centrifugal Filter Unit with Ultracel-10 membrane</td><td>Millipore Sigma</td><td>UFC501096</td><td>ultrafiltraton membrane for dialysis</td></tr><tr><td>Eppendorf 5417C Centrifuge</td><td>Marshall Scientific</td><td>EP-5417C</td><td>centrifuge</td></tr><tr><td>Myblock Mini Drybath</td><td>Benchmark Scientific</td><td>BSH200</td><td>drybath</td></tr><tr><td>FreeZone Plus 6 Liter Cascade Console Freeze Dry System</td><td>Labconco</td><td>7934020</td><td>lyophilizer</td></tr><tr><td>all priers and probes</td><td>IDT</td><td>custom</td><td>RT-LAMP primers and probes</td></tr><tr><td>dNTP set</td><td>Bioline</td><td>BIO-39049</td><td></td></tr><tr><td>Deoxyuridine Triphosphate (dUTP)</td><td>Promega</td><td>U1191</td><td></td></tr><tr><td>Bst&amp;nbsp;2.0 WarmStart&amp;nbsp;DNA Polymerase</td><td>New England Biolabs</td><td>M0538L</td><td>enzyme</td></tr><tr><td>WarmStart RTx Reverse Transcriptase</td><td>New England Biolabs</td><td>M0380L</td><td>enzyme</td></tr><tr><td>RNase Inhibitor, Murine</td><td>New England Biolabs</td><td>M0314L</td><td>enzyme</td></tr><tr><td>Antarctic Thermolabile UDG</td><td>New England Biolabs</td><td>M0372L</td><td>enzyme</td></tr><tr><td>50bp DNA Step Ladder</td><td>Promega</td><td>G4521</td><td>marker</td></tr><tr><td>LightCycler 480 Multiwell Plate 96, white</td><td>Roche Applied Science</td><td>4729692001</td><td>real-time RT-LAMP analysis</td></tr></tbody></table>

multiplexed isothermal amplification based diagnostic platform to detect zika, chikungunya, and dengue 1

Multiplexed Isothermal Amplification Based Diagnostic Platform to Detect Zika, Chikungunya, and Dengue 1

Zika, dengue, and chikungunya viruses are transmitted by mosquitoes, causing diseases with similar patient symptoms. However, they have different downstream patient-to-patient transmission potentials, and require very different patient treatments. Thus, recent Zika outbreaks make it urgent to develop tools that rapidly discriminate these viruses in patients and trapped mosquitoes, to select the correct patient treatment, and to understand and manage their epidemiology in real time.
Unfortunately, current diagnostic tests, including those receiving 2016 emergency use authorizations and fast-track status, detect viral RNA by reverse transcription polymerase chain reaction (RT-PCR), which requires instrumentation, trained users, and considerable sample preparation. Thus, they must be sent to &#34;approved&#34; reference laboratories, requiring time. Indeed, in August 2016, the Center for Disease Control (CDC) was asking pregnant women who had been bitten by a mosquito and developed a Zika-indicating rash to wait an unacceptable 2 to 4 weeks before learning whether they were infected. We very much need tests that can be done on site, with few resources, and by trained but not necessarily licensed personnel.
This video demonstrates an assay that meets these specifications, working with urine or serum (for patients) or crushed mosquito carcasses (for environmental surveillance), all without much sample preparation. Mosquito carcasses are captured on paper carrying quaternary ammonium groups (Q-paper) followed by ammonia treatment to manage biohazards. These are then directly, without RNA isolation, put into assay tubes containing freeze-dried reagents that need no chain of refrigeration. A modified form of reverse transcription loop-mediated isothermal amplification with target-specific fluorescently tagged displaceable probes produces readout, in 30 min, as a three-color fluorescence signal. This is visualized with a handheld, battery-powered device with an orange filter. Forward contamination is prevented with sealed tubes, and the use of thermolabile uracil DNA glycosylase (UDG) in the presence of dUTP in the amplification mixture.

Initially, the performances of each RT-LAMP primer (Table 1) with its corresponding viral RNA substrate as well as negative controls were assessed by gel electrophoresis. RT-LAMP primers were designed to target NS5 region (RNA-dependent RNA polymerase) for Zika and Dengue 1, and nsP2 region (non-structural protein P2) for Chikungunya. Templates were total RNA extracted from viral stocks cultured in African green monkey kidney (Vero) cells. In one case, total nucleic acid ...

Current multiplexed diagnostics to detect Zika, chikungunya, and dengue viruses require complex sample preparation and expensive instrumentation, and are difficult to use in low resource environments. We show a diagnostic that uses isothermal amplification with target-specific strand displaceable probes to detect and differentiate these viruses with high sensitivity and specificity.

Zika, dengue, and chikungunya viruses are transmitted by mosquitoes, causing diseases with similar patient symptoms. However, they have different ...

multiplexed-isothermal-amplification-based-diagnostic-platform-to

Research

JoVE Journal

Biochemistry

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.

A Multi-detection Assay for Malaria Transmitting Mosquitoes

This protocol describes the fabrication of a small, ready-to-use cassette that can be applied for visual detection of multiple nucleic acids in a single, test that is easy to operate. In this approach, a capillary array was used for multiplex and highly efficient detection of GMO targets.

Visual Detection of Multiple Nucleic Acids in a Capillary Array

In this protocol, we describe a technique to discover Zika virus specific diagnostic peptides using a high-density peptide microarray. This protocol can readly be adapted for other emerging infectious diseases.

Zika Virus Specific Diagnostic Epitope Discovery

This protocol provides an efficient and low-cost method to detect Zika virus or control targets in human urine and serum samples or in mosquitoes by reverse transcription loop-mediated isothermal amplification (RT-LAMP). This method does not require RNA isolation and can be done within 30 min.

Reverse Transcription-Loop-mediated Isothermal Amplification (RT-LAMP) Assay for Zika Virus and Housekeeping Genes in Urine, Serum, and Mosquito Samples

Presented here is a protocol for a fluorescence imaging approach, multiplex immunofluorescent cell-based detection of DNA, RNA, and protein (MICDDRP), a method capable of simultaneous fluorescence single-cell visualization of viral protein and nucleic acids of different type and strandedness. This approach can be applied to a diverse range of systems.

Single-Cell Multiplexed Fluorescence Imaging to Visualize Viral Nucleic Acids and Proteins and Monitor HIV, HTLV, HBV, HCV, Zika Virus, and Influenza Infection

Access to decentralized, low-cost, and high-capacity diagnostics that can be deployed into the community for decentralized testing is critical for combating global health crises. This manuscript describes how to build paper-based diagnostics for viral RNA sequences that can be detected with a portable optical reader.

Design to Implementation Study for Development and Patient Validation of Paper-Based Toehold Switch Diagnostics

We present two probe-based in-house one-step RT-qPCR kits for common respiratory viruses. The first assay is for SARS-CoV-2 (N), Influenza A (H1N1 and H3N2), and Influenza B. The second is for SARS-Cov-2 (N) and MERS (UpE and ORF1a). These assays can be successfully implemented in any specialized laboratory.

Development of Multiplex Real-Time RT-qPCR Assays for the Detection of SARS-CoV-2, Influenza A/B, and MERS-CoV

Multiplex fluorescence immunoassays are becoming a reference for serology testing. Their application, however, is limited by the complexity and time-consuming bead-analyte coupling processes. This report presents a semi-automated, reproducible multiplex microsphere bead coupling protocol that is comparable to the standard method while considerably reducing time to results.

A Multiplex Serological Assay for the Detection of Antibody Responses to Arboviruses

Nanoparticle-based optical probes have been designed as a vehicle for detecting antigens using Raman and UV-Vis spectroscopy. Here we describe a protocol for preparing such probes for a UV-Vis/Raman spectroscopy immunoassay in such a way to incorporate future multiplexing capabilities.

Fabricating a UV-Vis and Raman Spectroscopy Immunoassay Platform

Here we present a protocol of whole-cell electrochemical experiments to study the contribution of proton transport to the rate of extracellular electron transport via the outer-membrane cytochromes complex in Shewanella oneidensis MR-1.

Electrochemical Detection of Deuterium Kinetic Isotope Effect on Extracellular Electron Transport in Shewanella oneidensis MR-1

Learn a multiplexed point-of-care diagnostic method for detecting Zika, chikungunya, and dengue viruses using isothermal amplification with minimal sample preparation. This technique enables rapid virus detection in resource-limited settings.

Multiplexed Isothermal Amplification Based Diagnostic Platform to Detect Zika, Chikungunya, and Dengue 1

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