Name: Evaluation of Extracellular Vesicle Function During Malaria Infection (Video) | JoVE Journal
Uploaded: 2018-02-14T14:30:00.000+00:00
Duration: 13 min 45 s
Description: Learn to isolate and visualize extracellular vesicles from Plasmodium falciparum infected erythrocytes interacting with endothelial cells. This method reveals parasite-host communication mechanisms in malaria.

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5 minutes

This study was financially supported in part by the Novartis foundation for medical- and biological research (to PYM), the Gottfried and Julia Bangerter-Rhyner-Stiftung (to MW and PYM), and the research pool of the University of Fribourg (to PYM). Additional grants include the Swiss Government Excellence Scholarships for Foreign Scholars (to KAB and SM). We thank Isabelle Fellay and Solange Kharoubi Hess for technical support.

Human RBCs were obtained from the blood of healthy donors, in accordance with the guidelines of Swissethics (swissethics.ch).
NOTE: P. falciparum parasite cultures (3D7) and EV production were previously described in Mbagwu, et al.11 Because P. falciparum is a human pathogen, consult the local regulations for handling. The cultures should be kept sterile the entire time.
1. Fluorescence Labeling of EVs
NOTE: The following procedure takes advantage of the labeling technology to stably incorporate a green fluorescent dye (PKH67) with large aliphatic tails in the lipid region of the EV membrane. The reaction is performed in a 200 &#181;L final staining volume containing a 20 &#181;M final concentration of PKH67. Perform all steps at ambient temperature (20-25 &#176;C)
<ol>
	<li>Place 100 &#181;g of EVs in 1 mL of PBS in a microcentrifuge tube.</li>
	<li>Centrifuge the EVs in a microcentrifuge tube at maximum speed (20,000 x g) for 7 min to pellet. 
	NOTE: Since hemozoin is present in EVs, a red-dark brownish pellet should be observed. If the supernatant is reddish, then the EVs have lysed.</li>
	<li>After centrifugation, aspirate the supernatant carefully, in order to avoid removing any EVs. 
	NOTE: Minimize the amount of remaining buffer present before resuspending EVs in diluent C in order to increase reproducibility and efficiency of the staining.</li>
	<li>Resuspend the EV pellet in 100 &#181;L of diluent C (2X EV Suspension) and gently pipet to insure complete dispersion.</li>
	<li>Prepare a new microcentrifuge tube and add 4 &#181;L of the PKH67 ethanolic dye solution to 100 &#181;L of diluent C. Vortex well to mix. Prepare this 2x dye solution (40 &#181;M) immediately prior to staining. 
	NOTE: To avoid heterogeneous staining, do not add the PKH67 ethanolic dye solution directly to the EV pellet.</li>
	<li>Rapidly, combine the 100 &#181;L of 2X EV Suspension (step 1.4) with the 100 &#181;L of 2X dye solution (step 1.5). Then, mix the sample by pipetting up and down 10 times.</li>
	<li>Incubate the EV/Dye suspension from step 1.6 for 5 min protected from light and mix by vortexing 3-4 times during the 5 min incubation. 
	NOTE: Incubating the EV/Dye suspension for longer times provides no advantage, because the staining is so rapid.</li>
	<li>Stop the staining reaction by adding an equal volume (200 &#181;L) of serum and incubate for 1 min to allow binding of excess dye. 
	NOTE: Before stopping the staining, deplete the serum from EVs by centrifugation at 20,000 x g for 20 min.</li>
	<li>Wash 3 times with PBS and spin down at 20,000 x g for 5 min. Resuspend the EVs in 100 &#181;L of PBS to reach a final concentration of 1 &#181;g/&#181;L.</li>
</ol>
2. Visualize Uptake of EVs by Confocal Microscopy
NOTE: The following protocol describes the tracking of EV internalization by endothelial cells grown on glass coverslips. The endothelial cells are semi-immortalized human Bone Marrow Endothelial cells as described in12.
<ol>
	<li>Working in a sterile environment, coat coverslips with an excess of 0.01% poly-L-lysine for 10 min at room temperature (RT).</li>
	<li>Aspirate the poly-L-lysine solution and allow the coverslips to dry completely.</li>
	<li>Perform a viable endothelial cell count using Trypan blue exclusion and a hemocytometer.</li>
	<li>Transfer 1 x 105 endothelial cells in 1 mL of complete Endothelial Cell Growth Medium containing the Supplement Mix to the poly-L-lysine-coated coverslips and let the cells grow to a monolayer. 
	NOTE: The medium contains growth factors that allow cells to form a monolayer and to form tight junctions.</li>
	<li>Once the cells form a monolayer, carefully aspirate the medium and add 1 mL of fresh medium to wash the cells. Repeat the wash once more. Add 50 &#181;g of PKH67-labeled EVs and incubate for 4 h. 
	NOTE: To find the optimal time-point for uptake, a time-course can be performed.</li>
	<li>After 4 h, aspirate the medium, and wash the cells 3 times with PBS to remove excess and unbound EVs. Fix the cells with 3% paraformaldehyde solution in PBS for 15 min. 
	NOTE: Methanol can disrupt actin during the fixation process; therefore, it is best to avoid any methanol containing fixatives or other solvent-based fixatives. It is recommended to use methanol-free formaldehyde as a fixative.</li>
	<li>Wash the cells 3 times with PBS. Add carefully 250 &#181;L of 0.1% Triton X-100 in PBS to permeabilize the cells. Incubate at RT for 5 min.</li>
	<li>Wash 3 times with PBS. Add 400 &#181;L of blocking buffer (5% BSA in PBS) for 30 min at RT to block non-specific binding.</li>
	<li>Wash the cells once with PBS. Prepare the staining solution by diluting 5 &#181;L of the phalloidin stock solution in 200 &#181;L PBS/1% BSA per each cover slip. Pipet 200 &#181;L of the staining solution on the coverslip and incubate for 20 min at RT.</li>
	<li>Wash 3 times with PBS. Counterstain the DNA for 30 s with Hoechst 33342 at a final concentration of 2 &#181;g/mL in 200 &#181;L of PBS.</li>
	<li>Wash 2x the coverslip by adding 400 &#181;L of PBS. Carefully grab the coverslip with forceps and invert it on the top of a drop of antifade mounting media on a glass slide. Remove gently the excess media with a tissue and seal each side with nail polish.</li>
	<li>Store the slides protected from the light at 4 &#176;C.</li>
	<li>Visualize the cells using a confocal microscope at laser excitations 405, 488, and 543 nm and a 63X, 1.3 NA oil objective with fluorescent emissions at 450-470 nm (blue), 505-530 nm (green), and 620 nm. 
	NOTE: Typical F-actin staining results are shown in Figure 1.</li>
</ol>
3. Endothelial Cell Permeability
NOTE: Endothelial cell permeability is assessed by measuring the transfer of rhodamine B isothiocyanate-dextran (average MW 70,000) across the endothelial cell monolayer. Dextran provides an excellent tool to study vascular permeability.
<ol>
	<li>Count viable endothelial cells using 0.4 % Trypan blue exclusion and a hemocytometer.</li>
	<li>Plate the endothelial cells at a density of 0.6 x 105 cells to confluence in 24-well tissue culture inserts (0.4 &#181;m pore size) and leave undisturbed for at least 5 days to form differentiated monolayers. Refresh the medium every second day.</li>
	<li>Once the cells reach a monolayer, load the EVs (50 &#181;g in 1 mL) on the upper chamber. Add the rhodamine-dextran to the top well at a final concentration of 20 mg/mL. Incubate the cells at 37 &#176;C with 5% CO2.</li>
	<li>Monitor the transfer of the fluorescent dextran to the bottom well by measuring fluorescence emission from 40 &#181;L medium aliquots. Set up the multi-label microplate reader at 544 nm excitation and 590 nm emission for measurements. 
	NOTE: The amount of diffused dextran can be quantified using calibration curves established with the stock solution. In addition, kinetic experiments can be performed by removing small samples of the outer chamber medium during a time course (Figure 2). Even without any treatment, the dextran will diffuse through the cell monolayer.</li>
</ol>
4. Determine Puromycin Sensitivity
NOTE: Before transducing the cell lines with lentivirus, it is important to determine the kill curve of a selected drug for that particular cell line. To determine the minimum amount of drug concentration necessary to kill all of the cells, perform a dose response experiment using incremental doses of the selected drug. Because each mammalian cell line has a different sensitivity, before experimentation, the optimal concentration of the antibiotic should be determined by developing the kill curve titration as detailed below.
<ol>
	<li>Count the cells using the hemocytometer. Resuspend the endothelial cells at a concentration of 1 x 105 cells/mL in complete Endothelial Cell Growth Medium containing the Supplement Mix.</li>
	<li>Plate 1 x 104 cells into a 96-well plate in a final volume of 100 &#181;L of the Endothelial Cell Growth Medium.</li>
	<li>Add 100 &#181;L of medium containing the antibiotics to obtain a concentration of 0.1-10 &#181;g/mL (see Figure 3).</li>
	<li>Examine the cell viability every 2 days under a light microscope using a 20X objective. Culture the cells for 10-14 days and replace the media containing puromycin every 2-3 days depending on cell growth.</li>
	<li>Add 10 &#181;L/well MTS Reagent into each well, mix, and incubate for 4 h at 37 &#176;C in standard culture conditions.</li>
	<li>Shake the plate briefly on a shaker and measure absorbance of treated and untreated cells using a plate reader at 490 nm (Figure 3).</li>
</ol>
5. Transduction of Endothelial Cells with Lentiviral Vector
<ol>
	<li>Plate 1 x 105 endothelial cells in 1 mL of complete medium the day before transduction. Perform transduction when the cells have reached 50-80% confluency.</li>
	<li>Thaw the lentivirus on ice, and make aliquots of the viral stocks to avoid freeze-thaw cycles. Spin down the material at 200 x g for 30 s, in tubes before opening to avoid spill over.</li>
	<li>Add hexadimethrine bromide to the cells at a final concentration of 8 &#181;g/mL. 
	NOTE: Hexadimethrine bromide helps the transduction efficiency, however in some cases it might be toxic for the cells. Therefore, the optimal concentration should be determined by performing a killing curve before the transduction.</li>
	<li>Swirl the plate gently to mix. Add the appropriate quantity of viral particles (between 0.5-2 x 106 particles) at a suitable multiplicity of infection (MOI) and swirl the plate gently for 30 s to mix.</li>
	<li>Centrifuge the cell-viral particle mix in the centrifuge at RT for 45 min at 300 x g to increase the transduction efficiency. Incubate the cell-viral particle mixture at 37 &#176;C overnight.</li>
	<li>Remove carefully the viral particle-containing medium and discard appropriately. Replace it with fresh, pre-warmed complete culture medium.</li>
	<li>Start the selection with puromycin on the second day: remove the medium and replace it with fresh medium containing the correct concentration of puromycin as determined previously in section 4 (Figure 3).</li>
	<li>Harvest cells after puromycin selection and isolate RNA using an RNA isolating kit following the manufacturer&#39;s instructions.</li>
	<li>Perform cDNA synthesis with the selected miRNAs using a reverse transcription kit (see the Table of Materials).</li>
	<li>Set up the qPCR reaction according to the cited protocol13.</li>
</ol>

<ol><li>WHO. <a target="_blank" href="http://www.who.int/malaria/publications/world-malaria-report-2015/report/en/">WHO Malaria Report 2015</a>. , (2015).</li>
<li>Miller, L. H., Baruch, D. I., Marsh, K., Doumbo, O. K. <a target="_blank" href="https://www.ncbi.nlm.nih.gov/pubmed/11832955">The pathogenic basis of malaria.</a> Nature. 415 (6872), 673-679 (2002).</li>
<li>Mantel, P. Y., Marti, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((The+role+of+extracellular+vesicles+in+Plasmodium+and+other+protozoan+parasites%5BTitle%5D)+AND+%22Cell+Microbiol%22%5BJournal%5D)">The role of extracellular vesicles in Plasmodium and other protozoan parasites.</a> Cell Microbiol. 16 (3), 344-354 (2014).</li>
<li>Couper, K. N., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Parasite-derived+plasma+microparticles+contribute+significantly+to+malaria+infection-induced+inflammation+through+potent+macrophage+stimulation%5BTitle%5D)+AND+%22PLoS+Pathog%22%5BJournal%5D)">Parasite-derived plasma microparticles contribute significantly to malaria infection-induced inflammation through potent macrophage stimulation.</a> PLoS Pathog. 6 (1), e1000744(2010).</li>
<li>Schofield, L., Grau, G. E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Immunological+processes+in+malaria+pathogenesis%5BTitle%5D)+AND+%22Nat+Rev+Immunol%22%5BJournal%5D)">Immunological processes in malaria pathogenesis.</a> Nat Rev Immunol. 5 (9), 722-735 (2005).</li>
<li>Mantel, P. Y., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Malaria-infected+erythrocyte-derived+microvesicles+mediate+cellular+communication+within+the+parasite+population+and+with+the+host+immune+system%5BTitle%5D)+AND+%22Cell+Host+Microbe%22%5BJournal%5D)">Malaria-infected erythrocyte-derived microvesicles mediate cellular communication within the parasite population and with the host immune system.</a> Cell Host Microbe. 13 (5), 521-534 (2013).</li>
<li>Regev-Rudzki, N., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Cell-cell+communication+between+malaria-infected+red+blood+cells+via+exosome-like+vesicles%5BTitle%5D)+AND+%22Cell%22%5BJournal%5D)">Cell-cell communication between malaria-infected red blood cells via exosome-like vesicles.</a> Cell. 153 (5), 1120-1133 (2013).</li>
<li>Szempruch, A. J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Extracellular+Vesicles+from+Trypanosoma+brucei+Mediate+Virulence+Factor+Transfer+and+Cause+Host+Anemia%5BTitle%5D)+AND+%22Cell%22%5BJournal%5D)">Extracellular Vesicles from Trypanosoma brucei Mediate Virulence Factor Transfer and Cause Host Anemia.</a> Cell. 164 (1-2), 246-257 (2016).</li>
<li>Bartel, D. P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((MicroRNAs%3A+genomics%2C+biogenesis%2C+mechanism%2C+and+function%5BTitle%5D)+AND+%22Cell%22%5BJournal%5D)">MicroRNAs: genomics, biogenesis, mechanism, and function.</a> Cell. 116 (2), 281-297 (2004).</li>
<li>Mantel, P. Y., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Infected+erythrocyte-derived+extracellular+vesicles+alter+vascular+function+via+regulatory+Ago2-miRNA+complexes+in+malaria%5BTitle%5D)+AND+%22Nat+Commun%22%5BJournal%5D)">Infected erythrocyte-derived extracellular vesicles alter vascular function via regulatory Ago2-miRNA complexes in malaria.</a> Nat Commun. 7, 12727(2016).</li>
<li>Mbagwu, S., Walch, M., Filgueira, L., Mantel, P. Y. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Production+and+Characterization+of+Extracellular+Vesicles+in+Malaria%5BTitle%5D)+AND+%22Methods+Mol+Biol%22%5BJournal%5D)">Production and Characterization of Extracellular Vesicles in Malaria.</a> Methods Mol Biol. 1660, 377-388 (2017).</li>
<li>Schweitzer, K. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Characterization+of+a+newly+established+human+bone+marrow+endothelial+cell+line%3A+distinct+adhesive+properties+for+hematopoietic+progenitors+compared+with+human+umbilical+vein+endothelial+cells%5BTitle%5D)+AND+%22Lab+Invest%22%5BJournal%5D)">Characterization of a newly established human bone marrow endothelial cell line: distinct adhesive properties for hematopoietic progenitors compared with human umbilical vein endothelial cells.</a> Lab Invest. 76 (1), 25-36 (1997).</li>
<li>Wong, W., Farr, R., Joglekar, M., Januszewski, A., Hardikar, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Probe-based+Real-time+PCR+Approaches+for+Quantitative+Measurement+of+microRNAs%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Probe-based Real-time PCR Approaches for Quantitative Measurement of microRNAs.</a> J Vis Exp. (98), (2015).</li>
<li>Mulcahy, L. A., Pink, R. C., Carter, D. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Routes+and+mechanisms+of+extracellular+vesicle+uptake%5BTitle%5D)+AND+%22J+Extracell+Vesicles%22%5BJournal%5D)">Routes and mechanisms of extracellular vesicle uptake.</a> J Extracell Vesicles. 3, (2014).</li>
<li>French, K. C., Antonyak, M. A., Cerione, R. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Extracellular+vesicle+docking+at+the+cellular+port%3A+Extracellular+vesicle+binding+and+uptake%5BTitle%5D)+AND+%22Semin+Cell+Dev+Biol%22%5BJournal%5D)">Extracellular vesicle docking at the cellular port: Extracellular vesicle binding and uptake.</a> Semin Cell Dev Biol. 67, 48-55 (2017).</li>
<li>Montecalvo, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Mechanism+of+transfer+of+functional+microRNAs+between+mouse+dendritic+cells+via+exosomes%5BTitle%5D)+AND+%22Blood%22%5BJournal%5D)">Mechanism of transfer of functional microRNAs between mouse dendritic cells via exosomes.</a> Blood. 119 (3), 756-766 (2012).</li>
<li>Idro, R., Jenkins, N. E., Newton, C. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Pathogenesis%2C+clinical+features%2C+and+neurological+outcome+of+cerebral+malaria%5BTitle%5D)+AND+%22Lancet+Neurol%22%5BJournal%5D)">Pathogenesis, clinical features, and neurological outcome of cerebral malaria.</a> Lancet Neurol. 4 (12), 827-840 (2005).</li>
<li>Jambou, R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Plasmodium+falciparum+adhesion+on+human+brain+microvascular+endothelial+cells+involves+transmigration-like+cup+formation+and+induces+opening+of+intercellular+junctions%5BTitle%5D)+AND+%22PLoS+Pathog%22%5BJournal%5D)">Plasmodium falciparum adhesion on human brain microvascular endothelial cells involves transmigration-like cup formation and induces opening of intercellular junctions.</a> PLoS Pathog. 6 (7), e1001021(2010).</li>
<li>Zhou, W., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Cancer-secreted+miR-105+destroys+vascular+endothelial+barriers+to+promote+metastasis%5BTitle%5D)+AND+%22Cancer+Cell%22%5BJournal%5D)">Cancer-secreted miR-105 destroys vascular endothelial barriers to promote metastasis.</a> Cancer Cell. 25 (4), 501-515 (2014).</li>
</ol>

The authors have nothing to disclose.

Several parasites, including Toxoplasma, Trypanosoma, Leishmania, and Trichomonas trigger the release of EVs by the infected host cell. Depending on the pathogens, the released EVs can modulate the host immune response or mediate cellular communication between the parasites6. Yet, there is little evidence suggesting how these small vesicles contribute to malaria disease. Here, we have described several ways to investigate the function of EVs during Plasmodium infection. For instance, the ...

According to the World Health Organization, there were 212 million new cases of malaria worldwide in 2015 and approximately 429,000 people died, mainly children under five years of age1. The mechanisms leading to severe disease, which is often associated with vascular dysfunction, remain ill-defined2. Plasmodium-iRBCs secrete small bi-lipid membrane spheres known as extracellular vesicles (EVs). It is known that these EVs are potentially relevant to the infection process and to the host immune response to infection; however, little is known about the exact function of these small vesicles during malaria infection3. It is possible that they play two important roles: on one hand, they might contribute to the pathogenesis by activating macrophages4,5; and on the other hand, they might mediate cellular communication between parasites and between parasites and host6,7. In fact, parasites can transfer proteins or nucleic acids between each other via EVs. For example, Trypanosoma brucei rhodesiense EVs can transfer virulence factor Serum Resistance-Associated (SRA), and can target both other T. brucei and host erythrocytes8. Furthermore, P. falciparum-iRBCs communicate between each other by transferring nucleic acids within EVs. This allows the parasites to optimize and synchronize its growth. In fact, EVs might be the major regulator of gametocyte conversion, and therefore contribute to the regulation of the transmission stage7.
Not only do EVs regulate the parasites, they also mediate parasite-host interactions. We recently discovered that EVs from iRBCs contain host-derived microRNAs (miRNAs; small RNA species in the range of 21-25 nucleotides9) that were taken up by human endothelial cells. The miRNAs in the EVs form a stable complex with Ago2 (a member of the RNA-induced silencing complex), which once delivered to the recipient cells, is capable of specifically silencing gene expression and affecting the barrier properties of the cells10. Standard protocols have been developed to investigate the function of EVs. Here, we describe first a protocol that allows the fluorescent labeling of EVs to investigate their uptake by recipient cells. In addition, by using a confocal microscope, it is possible to track the EV&#39;s fate inside the cell. Several fluorescent dyes can be used to track EVs. The amine-reactive dye, 5-(and-6)-Carboxyfluorescein Diacetate Succinimidyl Ester (CFSE) and Calcein-AM become fluorescent once inside the vesicles. We prefer to use the amphiphilic label, PKH, because it gives a brighter and more uniform signal. This approach provides important information to understand the interactions between EVs and recipient cells. While in some cases EVs bind to the surface of the cells, some vesicles are rapidly taken up. Upon uptake, EVs deliver their cargoes to the cells, in which they exert their regulatory functions.
Here, we describe a protocol to measure the barrier function of the endothelial cells in vitro by quantifying the transfer of a fluorescent dextran through a cellular monolayer. More sensitive tracers can be used such as radiolabeled markers. However, they require special safety precautions for use. Other assays exist to measure the in vitro barrier function such as transendothelial electrical resistance (TEER), which measures tight junction integrity. Finally visualizing ZO-1, a tight junction protein, by immunofluorescence allows assessment of tight junction integrity as well10. Since EVs are complex and heterogeneous entities containing several cargoes with potential regulatory characteristic, it is useful to overexpress a specific RNA to study its effect on the recipient cell. Therefore, we also define a protocol that aims to generate stable cell lines expressing the miRNA of interest10.

<table><tbody><tr><td>PKH67 Green Fluorescent Cell Linker Mini Kit</td><td>Sigma-Aldrich</td><td>MINI67-1KT</td><td></td></tr><tr><td>Diluent C</td><td>Sigma-Aldrich</td><td>G8278</td><td></td></tr><tr><td>poly-L-lysine</td><td>Sigma-Aldrich</td><td>P8920</td><td></td></tr><tr><td>PBS</td><td>ThermoFisher - Gibco</td><td>10010023</td><td></td></tr><tr><td>Phalloidin CF594</td><td>Biotium</td><td>#00045</td><td></td></tr><tr><td>Hoechst 33342</td><td>ThermoFisher</td><td>H3570</td><td></td></tr><tr><td>ProLong Gold Antifade Mountant</td><td>ThermoFisher</td><td>P36934</td><td></td></tr><tr><td>Rhodamine B isothiocyanate&amp;ndash;Dextran</td><td>ThermoFisher</td><td>R9379-250MG</td><td></td></tr><tr><td>Insert with PET membrane transparent Falcon&amp;nbsp;for plate 24 wells</td><td>Falcon</td><td>353095</td><td></td></tr><tr><td>Endothelial Cell Growth&amp;nbsp;Medium MV</td><td>Promocell</td><td>C-22020</td><td></td></tr><tr><td>Puromycin dihydrochloride</td><td>Sigma-Aldrich</td><td>P9620-10ML</td><td></td></tr><tr><td>MTS Cell Proliferation Colorimetric Assay Kit</td><td>Biovision</td><td>K300-500</td><td></td></tr><tr><td>hexadimethrine bromide</td><td>Sigma-Aldrich</td><td>107689-10G</td><td></td></tr><tr><td>MISSION&amp;nbsp;Lenti microRNA, Human hsa-miR-451a</td><td>Sigma-Aldrich</td><td>HLMIR0583</td><td></td></tr><tr><td>MISSION Lenti microRNA, ath-miR416, Negative Control 1 Transduction Particles</td><td>Sigma-Aldrich</td><td>NCLMIR001</td><td></td></tr><tr><td>MISSION&amp;nbsp;Lenti microRNA, Human</td><td>Sigma-Aldrich</td><td>NCLMIR0001</td><td></td></tr><tr><td>Leica TCS SP5</td><td>Leica Microsystems</td><td></td><td></td></tr><tr><td>miRNeasy mini Kit</td><td>Qiagen</td><td>217004</td><td></td></tr><tr><td>TaqMan MicroRNA Reverse Transcription Kit 1000 reactions</td><td>ThermoFisher</td><td>4366597</td><td></td></tr><tr><td>hsa-mir-451a&amp;nbsp;RT/750 PCR rxns</td><td>ThermoFisher</td><td>001141</td><td></td></tr><tr><td>U6 snRNA</td><td>ThermoFisher</td><td>001973</td><td></td></tr><tr><td>TaqMan Universal Master Mix II, with UNG</td><td>ThermoFisher</td><td>4440038</td><td></td></tr><tr><td>StepOnePlus Real-Time PCR System</td><td>ThermoFisher</td><td>4376600</td><td></td></tr></tbody></table>

evaluation of extracellular vesicle function during malaria infection

Evaluation of Extracellular Vesicle Function During Malaria Infection

Malaria is a life-threatening disease caused by Plasmodium parasites, with P. falciparum being the most prevalent on the African continent and responsible for most malaria-related deaths globally. Several factors including parasite sequestration in tissues, vascular dysfunction, and inflammatory responses influence the evolution of the disease in malaria-infected people. P. falciparum-infected red blood cells (iRBCs) release small extracellular vesicles (EVs) containing different kinds of cargo molecules that mediate pathogenesis and cellular communication between parasites and host. EVs are efficiently taken up by cells in which they modulate their function. Here we discuss strategies to address the role of EVs in parasite-host interactions. First, we describe a straightforward method for labeling and tracking EV internalization by endothelial cells, using a green cell linker dye. Second, we report a simple way to measure permeability across an endothelial cell monolayer by using a fluorescently labeled dextran. Finally, we show how to investigate the role of small non-coding RNA molecules in endothelial cell function.

Here, we describe protocols to investigate the interactions of EVs with host cells. The uptake of fluorescently labeled EVs is monitored by confocal microscopy (Figure 1). Endothelial cells efficiently take up EVs, however the incubation time with EVs can be optimized to track the uptake. For a better localization of EVs inside the cells, stain actin with phalloidin. Next, we use a filter membrane on top of which a monolayer of endothelial cells grows. Rhodam...

In this work, we describe protocols to investigate the role of extracellular vesicles (EVs) released by Plasmodium falciparum infected erythrocytes. In particular, we focus on the interactions of EVs with endothelial cells.

Malaria is a life-threatening disease caused by Plasmodium parasites, with P. falciparum being the most prevalent on the African continent and responsible ...

evaluation-of-extracellular-vesicle-function-during-malaria-infection

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Isolation and Analysis of Brain-sequestered Leukocytes from Plasmodium berghei ANKA-infected Mice

Measuring antibody function is key to understanding immunity to Plasmodium falciparum malaria. This method describes the purification of viable merozoites, and measurement of opsonization-dependent phagocytosis by flow cytometry.

High Yield Purification of Plasmodium falciparum Merozoites For Use in Opsonizing Antibody Assays

The malaria parasite invades and replicates within red blood cells. The accurate assessment of merozoite invasion and parasitemia is therefore crucial in assessing the course of malaria infection. Here we describe a flow cytometry based protocol for the measurement of these parameters in a mouse model of malaria.

In Vivo Assessment of Rodent Plasmodium Parasitemia and Merozoite Invasion by Flow Cytometry

Human co-infection is difficult to replicate in vitro. However, human malaria parasites can readily be cultured in vitro, as can freshly isolated human peripheral blood mononuclear cells naturally infected with HIV. This provides an excellent model for studying early immune responses to malaria parasites in the context of HIV co-infection.

An In Vitro Model for Measuring Immune Responses to Malaria in the Context of HIV Co-infection

Human microRNAs translocate from host erythrocytes to Plasmodium falciparum parasites. Here, the techniques used to transfect synthetic microRNAs into host erythrocytes and isolate all RNAs from P. falciparum are described.  In addition, this paper will detail a method of polysome isolation in P. falciparum to determine the ribosomal occupancy and translational potential of parasite transcripts.

Methods to Investigate the Regulatory Role of Small RNAs and Ribosomal Occupancy of Plasmodium falciparum

We describe here a protocol for isolating myeloid cells from mouse skin and draining lymph node following intradermal injection of Plasmodium sporozoites. Flow cytometry of collected cells provides a reliable assay to characterize the skin and draining lymph node inflammatory response to the parasite.

Myeloid Cell Isolation from Mouse Skin and Draining Lymph Node Following Intradermal Immunization with Live Attenuated Plasmodium Sporozoites

The overall goal of this protocol is to provide instruction on how to measure the capacity of antibodies present in sera or plasma of individuals, naturally exposed to Plasmodium falciparum infection, to opsonize and induce phagocytosis of the parasite-infected erythrocytes (IEs).

Measuring Naturally Acquired Phagocytosis-Inducing Antibodies to Plasmodium falciparum Parasites by a Flow Cytometry-Based Assay

Here we describe a new method to help elucidate the mechanisms of cellular immunity to Plasmodium during the blood stage of infection. This is an in vitro assay that measures infected red blood cell killing by cytotoxic...

In Vitro Assay of Plasmodium-Infected Red Blood Cell Killing by Cytotoxic Lymphocytes

Learn to isolate and visualize extracellular vesicles from Plasmodium falciparum infected erythrocytes interacting with endothelial cells. This method reveals parasite-host communication mechanisms in malaria.

Evaluation of Extracellular Vesicle Function During Malaria Infection

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