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

Summary

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 lymphocytes. 

Abstract

Malaria is a major public health concern, presenting more than 200 million cases per year worldwide. Despite years of scientific efforts, protective immunity to malaria is still poorly understood, mainly due to methodological limitations of long-term Plasmodium culture, especially for Plasmodium vivax. Most studies have focused on adaptive immunity protection against malaria by antibodies, which play a key role in controlling malaria. However, the sterile protection induced by attenuated Plasmodium sporozoites vaccines is related to cellular response, mainly to cytotoxic T lymphocytes, such as CD8⁺ and gamma delta T cells (γδ T). Hence, new methodologies must be developed to better comprehend the functions of the cellular immune response and thus support future therapy and vaccine development. To find a new strategy to analyze this cell-mediated immunity to Plasmodium blood-stage infection, our group established an in vitro assay that measures infected red blood cell (iRBC) killing by cytotoxic lymphocytes. This assay can be used to study cellular immune response mechanisms against different Plasmodium spp. in the blood stage. Innate and adaptative cytotoxic immune cells can directly eliminate iRBCs and the intracellular parasite in an effector:target mechanism. Target iRBCs are labeled to evaluate cell viability, and cocultured with effector cells (CD8⁺ T, γδ T, NK cells, etc.). The lysis percentage is calculated based on tested conditions, compared to a spontaneous lysis control in a flow cytometry-based assay. Ultimately, this killing assay methodology is a major advance in understanding cell-mediated immunity to blood-stage malaria, helping uncover new potential therapeutic targets and accelerate the development of malaria vaccines.

Introduction

Malaria remains a global health crisis, with more than 240 million cases and 627,000 malaria-related deaths reported in 2020¹. There are currently five parasitic species that can cause malaria in humans, out of which Plasmodium falciparum and Plasmodium vivax are the two most prevalent species. During Plasmodium infection, the liver or pre-erythrocytic stage is asymptomatic, and symptoms only occur during the parasite's asexual cycle in the erythrocytic stage. At this infection stage, thousands of merozoites derived from the liver stage are released into the bloodstream and infect red blood cells (RBCs). In the RBC, the parasites differentiate into trophozoites and schizonts by schizogony, until schizonts rupture the erythrocyte, releasing newly formed merozoites, repeating this blood cycle. Repeated cycles of invasion, replication, and merozoite release result in an exponential growth of the parasite population and ultimately trigger disease symptoms².

An important challenge in studying the immune response to malaria is that the Plasmodium spp. that infects humans does not infect laboratory animal models. Thus, Plasmodium-infected patient samples must be collected fresh and immediately processed and analyzed. However, in malaria-endemic areas, resources to access immunological and molecular mechanisms are limited. Due to these limitations, rodents are widely used as experimental models to investigate the immune response against Plasmodium infection. While P. berghei and P. chabaudi are often used as surrogates for P. falciparum infection, the non-lethal strain of P. yoelii 17XNL also has many features in common with P. vivax, such as reticulocyte restricted infection^3,4. The development of Plasmodium in vitro assays, that can be used for human or animal model-derived samples, is valuable in gaining a better understanding of the pathogenesis of malaria and comparing the immunological response elicited by different species of the parasite.

Protective antimalarial immunity is not completely understood either at the pre-erythrocytic stage nor the blood stage. It is known that exposure to repeated infections results in partial acquired immunity, but sterile immunity is rarely developed⁵. For decades, anti-Plasmodium protective immunity was mainly associated with the induction of neutralizing or opsonizing antibodies that prevent parasite invasion of host cells or lead to phagocytosis by antigen-presenting cells, respectively⁶. As a result, most efforts to produce antimalarial vaccines thus far have relied on inducing protective and long-lasting antibodies^7,8. However, the sterile protection induced by vaccination with an attenuated sporozoite directly correlates with the activation and expansion of cytotoxic T lymphocytes^8,9.

Recently, some studies of freshly isolated patient samples and in vitro cultures have demonstrated that innate or adaptative cytotoxic immune cells like CD8⁺ T¹⁰, γδ T¹¹, and NK cells¹² can directly eliminate Plasmodium-infected RBCs and its intracellular parasite in an effector:target ratio manner. These seminal findings defined an entirely new immune effector mechanism in the context of malaria. To dissect this novel antimalarial immunity, it is essential to explore cytotoxic effector mechanisms of killer cells against infected-RBCs (iRBCs) in natural infection or vaccination.

Here we present an in vitro assay that measures the cytotoxic activity of lymphocytes against malaria in the blood stage. This assay can then help elucidate the mechanisms of the cellular immune response against the Plasmodium erythrocyte stage. The target cells, iRBCs, are labeled with carboxyfluorescein succinimidyl ester (CFSE) to evaluate cell viability, and are then cocultured with effector cells like cytotoxic lymphocytes (CTL). This coculture is then evaluated by flow cytometry, using fluorescent markers for specific cell types. Finally, the percentage of iRBC lysis by CTL is calculated by dividing the experimental condition by the spontaneous rupture of RBCs and spontaneous lysis control, which occurs during incubation without the effector cell. Overall, this killing assay methodology can contribute to a better understanding of cell-mediated malaria immunity.

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Protocol

All procedures were conducted following the policies of the Oswaldo Cruz Foundation and the National Ethical Council (CAAE: 59902816.7.0000.5091). The human protocols were developed in collaboration with the clinical research group from the Research Center for Tropical Medicine of Rondônia (CEPEM), which was in charge of enrolling patients in the study. Informed consent was obtained from all the patients.

For the animal study, procedures were performed following the principles of conduct of the Brazilian Practice Guide for the Care and Use of Animals for Scientific and Didactic Purposes of the National Council for the Control of Animal Experimentation (CONCEA). The protocols were approved by the Fiocruz Animal Experimentation Council (CEUA protocol LW15/20-2).

1. Collection of human blood samples and PBMC isolation

1. Collect blood of Plasmodium-infected patients in a 10 mL evacuated blood collection tube with sodium heparin. As malaria patients display lymphopenia, there is a range of 5-9 x 10⁶ peripheral blood mononuclear cells (PBMCs) in a 10 mL blood sample. Since CD8⁺ T cells or γδ T cells make up ~10% of PBMCs, preferably collect 50-100 mL of blood/patient.
   NOTE: A minimum of 1 x 10⁵ effector cells/ condition should be considered.
2. Calculate the percentage of iRBCs by blood smear as described below.
   1. Add 5 μL of total blood to a clear slide and prepare a blood smear. Perform Romanowsky-type panoptic fast stain or May-Günwald-Giemsa stain. Here, the panoptic fast stain kit is used, which is composed of three reagents: reagent A (fixation), reagent B (cytoplasmic stain), and reagent C (nuclear and cytoplasmic differential stain).
   2. Slowly dip the slide in solution A 10x, then 4x in solution B, and finally 10x in solution C. Drain out any excess reagent from the slides between solutions. After dipping in solution C, rinse the slide in running tap water and let it dry.
   3. Under an upright light microscope with a 100x oil immersion objective, count 1000 RBCs in sequential squares and calculate the percentage of parasitemia using the following equation:
      
3. Dilute 15 mL of blood in a 1:1 proportion in sterile phosphate-buffered saline (PBS).
4. Add 15 mL of lymphocyte separation medium (density of 1.077g/mL) to a 50 mL tube. Carefully layer the 30 mL of diluted blood sample onto the centrifugation medium solution. When layering the sample, do not let the blood sample and lymphocyte separation medium mix.
5. Centrifuge the tubes at 400 x g for 40 min at 22 °C, with low acceleration and no break setting.
6. Draw off the upper layer containing plasma using a sterile pipette, leaving the mononuclear cell layer undisturbed. Transfer the layer of mononuclear cells (PBMCs) to a sterile tube using a sterile pipette.
7. Do not discard the tube containing the blood pellet as it will be used later for infected RBC isolation. From this step, be sure to keep the RBCs at room temperature (RT). Never let them cool down.
8. Wash the cells twice by adding PBS and centrifuge at 350 x g for 10 min, with break setting. Resuspend the cell pellet in 5 mL of RPMI medium supplemented with penicillin/streptomycin and 10% fetal bovine serum (FBS; complete medium).
9. Count the PBMCs in the presence of trypan blue solution to check cell viability, using a hemacytometer (Neubauer chamber) or automated cell counter. Do not count the blue-stained cells as these represent dying cells, which absorb trypan blue.
10. Adjust the cell concentration to 10⁷ cells/mL using complete medium. Purify the desired cytotoxic lymphocyte populations (CD8⁺ T cells, NK cells, γδ T cells) using magnetic beads isolation as per reagent manufacturer protocol.

2. Human RBC isolation

NOTE: For human-infected RBC isolation, it is recommended to start with blood samples that have a minimum of 2% parasitemia, preferentially with more in the trophozoite/early schizont parasite stage.

1. Prepare the PERCOLL (from hereafter referred to as density gradient separation medium) at the recommended concentration as described below.
   1. Add 90 mL of 100% density gradient separation medium and 10 mL of 10x PBS to obtain 90% isotonic density gradient separation medium.
   2. For P. vivax-infected reticulocyte separation, prepare45% density gradient separation media. Add 50 mL of 90% isotonic density gradient separation medium and 50 mL of 1x PBS to obtain 45% density gradient separation medium.
   3. For P. falciparum-infected erythrocyte separation, prepare 65% density gradient separation media. Add 72 mL of 90% isotonic density gradient separation medium and 28 mL of 1x PBS to obtain 65% density gradient separation medium.
   4. For uninfected reticulocyte separation, prepare 70% density gradient separation media. Add 78 mL of 90% isotonic density gradient separation medium and 22 mL of 1x PBS to obtain 70% density gradient separation medium.
2. Warm the density gradient separation medium to 37 °C in a water bath.
3. After removal of the PBMC layer, carefully remove as much of the top layer of centrifugation medium as possible without touching the cells. With a glass Pasteur pipette, carefully remove the upper neutrophil layer without disturbing the RBC pellet and estimate pellet volume. Add 4x the RBC pellet volume of RT complete medium and resuspend.
4. In a second 50 mL conical tube, add 5x the pellet volume of 45%, 65%, or 70% density gradient separation medium depending on the cell type to isolate. Layer the RBC suspension on top of the density gradient separation medium layer carefully.
5. Spin for 15 min at 850 x g, with low acceleration and no break setting. Collect the cloudy red/brown layer lying in between the supernatant and density gradient separation medium with a 5 mL pipette. Transfer to a sterile 15 mL tube.
6. Wash the cells by adding RT complete medium up to 15 mL and spin down for 10 min at 860 x g. Repeat the washing by adding 10 mL of RT complete medium and spin down. Discard the supernatant and prepare a blood smear from the pellet to check for iRBC enrichment, following step 1.2.
7. Resuspend the pellet in 1 mL of RT complete medium and let sit at room temperature while counting the cells. Add 10 μL of cell suspension in a hemocytometer (Neubauer chamber) and count the RBCs in the central area subdivided into 25 medium squares. Adjust cell concentration to 1 x 10⁷ iRBCs/mL in RT complete media.

3. Experimental malaria infection in mouse

1. Thaw an aliquot of cryopreserved P. yoelii 17XNL:PyGFP (MRA-817), a GFP-expressing strain obtained from MR4/ATCC, and inject 100 μL intraperitoneally (i.p.) in an 8-week-old female C57BL/6 mouse.
2. Follow the parasitemia burden every 3 days by tail vein lancing blood collection.
   1. Puncture the vessel with the needle bevel up, entering the vein at a shallow angle beginning at the distal end of the tail.
   2. Collect the blood sample with a pipette or capillary tube up to 5 or 10 mL, then apply manual pressure to stop the bleeding.
   3. Prepare a blood smear (as described in step 1.2) until parasitemia reaches 10%-15% of infected RBCs.
3. Collect 10 μL of blood by tail vein lancing and dilute to 100 μL of PBS to i.p. inject into the second donor mouse.
   NOTE: Cryopreserved parasites should be thawed and passed in mice twice before being used for experimental infections.
4. When the second passage reaches 15% of parasitemia, collect five drops of blood by the tail clipping method and dilute in 1 mL of PBS. Prepare an infection solution by adjusting the concentration to 1 x 10⁶ iRBCs/mL in sterile PBS and inject i.p. 100 μL (1 x 10⁵ iRBCs) of the solution into each mouse required for the experiment.
5. Monitor parasitemia every 2-3 days until it reaches ~30% iRBCs, which occurs approximately 12 days post-infection. When the mice reach the desired parasitemia, collect blood by cardiac puncture as described below.
   1. Aspirate 100 µL of heparin solution (30 U/mL) into a 1 mL syringe with a 26 G needle.
   2. Anesthetize the mouse by inhalation with 5% isoflurane and confirm the absence of reflexes. Place the mouse on its side and perpendicularly insert the needle just below the elbow, through the ribs, and into the heart. Pull out the syringe plunger slowly and rotate the needle until 0.5-1 mL of blood is obtained.
   3. Perform humane euthanasia by cervical dislocation under anesthesia. Aseptically clean the left side of the mouse with 70% ethanol. With surgical scissors, make a cut on the left side of the mouse passing through the skin and peritoneum. Locate the spleen and remove it.
   4. Place the mouse spleen in a Petri dish with 5 mL of complete medium to purify the desired effector cell population (e.g., CD8⁺ T cells).

4. Obtaining fresh whole mouse splenocytes

1. In the Petri dish, carefully cut the spleen into small pieces using scissors or a razor.
2. Place a 100 µM cell strainer over a 50 mL conical tube and transfer the excised spleen into the cell strainer with a pipette. Mash the spleen through the strainer with a syringe plunger.
3. Wash the cells through the strainer with 10 mL of complete media. Centrifuge the cells at 300 x g for 10 min at 4 °C, then discard the supernatant.
4. Resuspend the cell pellet in 2 mL of cold 1x RBC lysis buffer. Incubate the suspension for 5 min on ice.
5. Wash the cell suspension with 10 mL of 4 °C complete media. Repeat the wash step three times and remove any cell clots between washes for spleens from Plasmodium-infected mice.
6. Centrifuge the cells at 400 x g for 5 min at 4 °C, then discard the supernatant.
   NOTE: Plasmodium-infected spleens are enlarged and filled with phagocytic cells containing degraded hemoglobin and hemozoin.
7. To avoid any issues during the magnetic bead isolation of effector cells, use the following steps to remove hemozoin-enriched phagocytic cells and hemozoin. Resuspend the splenic cells with MACS buffer and adjust concentration to 1 x 10⁸ cells/mL. Place an LS or LD column in the magnetic field. Prepare the column by rinsing with 3 mL of MACS buffer.
8. Apply cell suspension onto the column. Wash the column three times with 3 mL of MACS buffer. Collect flow-through containing the splenic cells.
9. Count the splenocytes in a trypan blue solution and check cell viability in a hemacytometer (Neubauer chamber) or automated cell counter. Adjust cell concentration to 1 x 10⁷ cells/mL in RT complete media.

5. Cytotoxic effector cell purification (CD8a⁺ T cell negative selection)

NOTE: There are many positive and negative selection reagents that can purify cytotoxic effector cells (CD8⁺ T, γδ T, NK, iNKT, MAIT cells). In this protocol, we use a negative selection of splenic CD8a⁺ T cells and follow manufacturer instructions.

1. Centrifuge all splenocytes at 400 x g for 10 min at 4 °C and discard the supernatant. Resuspend the cell pellet in 40 µL of MACS buffer.
2. Add 10 µL of a biotin-antibody cocktail. Mix well and incubate for 5 min on ice.
3. Add 30 µL of MACS buffer. Add 20 µL of anti-biotin micro-beads. Mix well and incubate for 10 min on ice.
4. Add 400 µL of MACS buffer and proceed to magnetic cell separation. Place the MACS LS column in the magnetic field support. Prepare the column by rinsing with 3 mL of MACS buffer.
5. Apply cell suspension onto the column. Wash the column three times with 3 mL of MACS buffer. Collect the flow-through containing all unlabeled cells, which are the enriched CD8a⁺ T cells.
6. Count the CD8a⁺ T cells in a trypan blue solution and check cell viability in a hemacytometer (Neubauer chamber) or automated cell counter. Adjust the cell concentration to 1 x 10⁷ cells/mL in RT complete media.

6. P. yoelii infected RBC isolation

1. Centrifuge the collected blood in a 1.5 mL tube at 850 x g for 3 min. Discard the serum and resuspend the blood in 1 mL of 1x RPMI without FBS.
2. Place the LS column in the magnetic field support and rinse with 3 mL of 1x RPMI. Pass the RBC suspension through the column. To isolate more iRBCs, reapply the flowthrough (3 mL of RPMI and 1 mL of diluted blood) into the column.
3. Wash twice with 5 mL of 1x RPMI. Perform washing steps by adding buffer aliquots as soon as the column reservoir is empty. Do not let any columns dry up.
4. Add 5 mL of RPMI, remove the column, and purge the iRBCs into a new 15 mL tube. Count the iRBCs and adjust the concentration to 1 x 10⁷ RBCs/mL.

7. CFSE labeling of RBCs and preparation for flow cytometry

NOTE: Start the RBC labeling protocol with twice the number of cells that will be used for the experiment, since ~50% of the cells are typically lost in the washing steps following the CFSE labeling step. To establish the autofluorescence of the RBCs/iRBCs, include a control sample of unlabeled cells.

1. Dilute CFSE to a final concentration of 10 mM in 1x RPMI without FBS. Wash the cells once with 1x RPMI without FBS in a 15 mL tube.
2. Resuspend the RBCs in 500 μL of 1x RPMI without FBS and add 500 μL of the diluted CFSE. Incubate for 8 min at RT, protected from light.
3. Wash three times by adding 14 mL of complete medium (10% FBS RPMI), followed by centrifugation at 850 x g for 10 min. Resuspend the cells in complete medium to a concentration of 1-5 x 10⁶/ mL. Incubate for 1 h at RT.

8. Cytotoxic lymphocyte/RBC coculture and preparation for flow cytometry

NOTE: If the involvement of specific receptors or molecules will be measured, incubate the specific blocking and isotype control antibodies (10 mg/mL) with the effector cells for 30 min before coculture.

1. Plate the cells in a 96-well round-bottom plate. Add the purified lymphocytes and CFSE-labeled iRBCs in the desired effector-target cell ratio to a final volume of 200 μL and homogenize. Prepare each condition in triplicate.
   NOTE: We suggest adjusting the iRBC concentration to 1-5 x 10⁴ cells/mL and choosing the ratio based on the purified cell number (e.g., 0.5:1, 2.5:1, and 5:1).
2. Include the spontaneous lysis control, which is the target iRBCs without the effector, to evaluate any spontaneous lysis, as this will be used to represent a 100% cell viability condition.
3. Spin down the plate for 1 min at 360 x g to maximize cell contact. Incubate at 37 °C and 5% CO₂ for 4 h.
   NOTE: Hypoxia conditions (low O₂), systematically used for P. falciparum culture, should not be used since the effector cells do not survive in this environment. In contrast, Plasmodium parasites are viable in ambient air in 5% CO₂ for up to 12 h.
4. Spin for 5 min at 850 x g and flip the plate to remove the supernatant.
   NOTE: If desired, the supernatant can be used to measure any soluble factors released in the coculture.
5. Label the RBCs with anti-mouse Ter119 1:200 (or anti-human CD235 1:100 for human samples) and CD8⁺ T cells with anti-CD8 1:200 or anti-CD3 1:200 antibodies (anti-mouse or human) for 30 min at 4 °C in 1x PBS containing 3% FBS (FACS buffer).
   NOTE: The antibody fluorophore should be selected based on the cell tracer/cell proliferation reagent (e.g., CFSE-labelled iRBC, APC-Cy7 anti-Ter119, and PerCP-Cy5.5 anti-CD8a).
6. Wash the cells with FACS buffer and spin down for 5 min at 850 x g. Transfer the samples to FACS tubes and add 30 μL of counting beads to individual tubes. Homogenize the count beads by vortexing for 30 s.

9. Flow cytometry

1. Analyze samples using a 405/488/561/640 laser instrument.
2. For human cells labeled with CFSE (FITC), PE anti-human γδ TCR, and PE-Cy7 anti-human CD235a antibody, use 530/30 (FITC), 575/25 (PE), and 780/60 (PE-Cy7) filters in a three-laser (Blue, Red, Yellow-Green) configuration cytometer.
3. For mouse cells labeled with CFSE (FITC), PerCP-Cy5.5 anti-mouse CD8a, and APC-Cy7 anti-mouse Ter119, use 530/30 (FITC), 695/40 (PerCP-Cy5.5), and 780/60 (APC-Cy7) filters in the three-laser cytometer setup.
4. Choose the counting beads population as the stopping gate to acquire a minimum of 20,000 events in the stop gate, which should be identical for all conditions. Perform analysis and compensation using appropriate flow cytometry acquisition/analysis software.
5. Set the gating strategy as described below.
   1. Select single cells (singlets), excluding debris using FSC peak height (H) to area (A) ratio. Select RBCs and exclude the lymphocytes from analysis based on fluorescence of the RBC marker (Ter119 or CD235a) and the lymphocyte-specific antibody (CD8a).
   2. In the previous RBC gating, select viable RBCs based on CFSE positive staining. Analyze the data with flow cytometer data analysis software.

10. Calculation and statistics

1. To calculate the percentage of iRBC lysis, follow the gating strategy described in step 9. The percentage of viable RBCs is the frequency of CFSE-positive cells inside the RBC gate based on Ter119 (mouse) or CD235a (human) positive fluorescence.
2. Use the spontaneous lysis control, RBCs without effector cells, condition as a control to estimate RBC spontaneous rupture. This condition will be considered RBC lysis (100% viability). Use the following formula to calculate the percentage of RBC lysis in each tested condition:
   
   NOTE: During the culture incubation, some infected RBCs may spontaneously lyse or be ruptured by the parasite. Use the CFSE-positive RBC frequency of the spontaneous lysis condition, which contains no effector cells, as the baseline for lymphocyte cytotoxicity.
3. Calculate the average of triplicates for each condition and determine statistical significance using two-way ANOVA at multiple comparisons.

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Results

Here, the applied methodology for isolation of CFSE-labeled Plasmodium-infected RBCs in a coculture assay with cytotoxic lymphocytes is described. First, we provide a schematic representation of how to perform the protocol, employing human samples infected with P. vivax (Figure 1). Then, an illustrated flowchart on how to proceed with the protocol in a malaria experimental model using a C57BL/6 mouse infected with P. yoelii (Figure 2)....

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Discussion

Here we describe an in vitro assay to measure Plasmodium-infected red blood cell killing by cytotoxic lymphocytes. This assay can help elucidate the mechanisms of cellular protective immunity to the malaria parasite's erythrocytic stage. The major advantage of this methodology is that it provides a quantitative assay of the cell-mediated killing of iRBCs that can be used to address many questions about how immune cells interact with different Plasmodium spp.

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Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
100 μM cell strainer	Corning	431752
96 Well Round (U) Bottom Plate	Thermo Scientific	12-565-65
Anti-human CD235a (Glycophorin A) Antibody	Biolegend	349114	Used - APC anti-human CD235, dilution 1:100
Anti-human CD3 Antibody	Biolegend	317314	Used - PB anti-human CD3, dilution 1:200
Anti-human CD8 Antibody	Biolegend	344714	Used - APC/Cy7 anti-human CD8, dilution 1:200
Anti-human TCR Vδ2 Antibody	Biolegend	331408	Used - PE anti-human TCR Vδ2, dilution 1:200
Anti-mouse CD8a Antibody	Biolegend	100733	Used- PerCP/Cyanine5.5 anti-mouse CD8a, dilution 1:200
Anti-mouse TER-119/Erythroid Cells Antibody	Biolegend	116223	Used - APC/Cyanine7 anti-mouse TER-119, dilution 1:200
CellTrace CFSE Cell Proliferation Kit	Invitrogen	C34554
Fetal Bovine Serum, qualified	Gibco	26140079
Ficoll-Paque Plus	Cytiva	17144003	Lymphocyte Separation Medium (LSM)
Heparin Sodium Injection, USP	meithel pharma	71228-400-003	Used - 2000 USP units/2mL
Isoflurane	Piramal critical care	66794-0013-25
LS MACS Column	Miltenyi Biotec	130-042-401
LSRFortessa Cell Analyzer	BD Bioscience
Percoll	Cytiva	17089101	Density Gradient Separation Medium (DGSM)
QuadroMACS Separator	Miltenyi Biotec	130-090-976
RPMI 1640 Medium	Gibco	11875093
Sodium bicarbonate, powder,  BioReagent	Sigma-Aldrich	S5761
Syringe With Sub-Q needle - 1mL, 26 gauge;	BD	14-829-10F
Vacutainer Heparin Tube Glass Green 10 ml	BD	366480