A Flow Cytometry Assay to Identify Immune Cell Subsets in Peripheral Blood Mononuclear Cells

Published: February 29, 2024

Abstract

Source: Torchia, M. L. G., et al. Discrimination of Seven Immune Cell Subsets by Two-fluorochrome Flow Cytometry. J. Vis. Exp. (2019)

This video demonstrates a flow cytometry-based technique using two fluorochromes to identify CD4+ and CD8+ T cells, γδ T cells, B cells, natural killer (NK) cells, and monocytes in human peripheral blood mononuclear cells (PBMCs). Upon incubating the cells with fluorochrome-conjugated antibodies against the surface markers, the cell subsets are identified using an optimal flow cytometric gating strategy.

Protocol

All procedures involving sample collection have been performed in accordance with the institute's IRB guidelines.

NOTE: This protocol has been tested on freshly or frozen isolated peripheral blood cells and whole blood.

1. Cell Staining

NOTE: Choosing pairs of fluorochromes with virtually no spectral overlap is important to reduce the spread of data due to the high spillover of a fluorochrome in the other fluorochrome detector. To achieve an optimal identification of all the cell subsets, fluorochromes with a high quantum yield should be used such as antibody pairs PE-BV421 and PE-APC.

  1. Staining of fresh and frozen PBMC
    1. Transfer 100 µL of PBMC (1 x 106 cells) to a 96-well V-bottom plate.
      NOTE: Any number of cells lower than 1 x 106 can be used with similar results.
    2. Centrifuge at 350 x g for 3 min at RT and carefully aspirate the supernatant without disturbing the cell pellet. Add to each well 100 µL of phosphate-buffered saline (PBS) containing a live/dead fixable dye that reacts with free amine on proteins for 10 min to label dead cells.
    3. Prepare for each sample 30 µL of a mix containing all the antibodies (anti-CD3. -CD56, TCRγδ in fluorochrome A, and anti-CD4, CD8, CD19, CD14 in fluorochrome B). The concentrations of antibodies are indicated in Table 1 and Table 2. At this stage, titrated antibodies against different target molecules and in different fluorochromes can be added as well (e.g., Table 3).
      NOTE: Antibodies concentration can vary depending on the manufacturer and lot number. Therefore, preliminary tests should be done to achieve the optimal signal. PBS, PBS/0.5% bovine serum albumin (BSA), PBS/0.2% sodium azide or PBS/0.5% BSA/0.1% sodium azide were used with similar results to dilute antibodies. Cells can also be stained in volumes different from 30 µL to easily integrate this methodology into already existing staining protocols.
    4. Centrifuge at 350 x g for 3 min at RT and carefully aspirate the supernatant without disturbing the cell pellet. Add the antibody cocktail to each well and resuspend carefully without generating bubbles. Incubate for 30 min at RT in the dark.
      NOTE: It is possible to stain the samples at 4 °C with similar results.
    5. Add 150 µL of staining buffer and centrifuge at 350 x g for 3 min at RT and carefully aspirate the supernatant without disturbing the cell pellet. Resuspend the cells in 200 µL of PBS and acquire data on a flow cytometer. If staining volumes are changed, please ensure at least a 20-fold dilution of the original antibody mix used to wash the excess antibodies.
      NOTE: Stained cells can be fixed within PBS/2% paraformaldehyde, kept in a refrigerator at 4 °C overnight, and then acquired on a flow cytometer the following day.
      CAUTION: Paraformaldehyde is harmful if swallowed and can cause skin irritation

2. Antibody Titration

NOTE: Antibody titration is the most critical step for obtaining high-quality, reproducible data. Titration of anti-CD3, -CD8, -CD14, -CD19, and -TCR γδ follows the standard procedure by which the concentration of antibody to optimally separate positive and negative peaks is derived by maximum staining index. Dilutions at the peak or closer to the peak on the rising side of the stain index curve should be selected (Figure 1A-C). The anti-CD4 antibody is titrated to place the peak of the CD4 positive population between CD3 single positive populations and CD3+/CD8+ T cells, closer to the CD3 single-positive signal to better discriminate the CD8dim populations (CD8+ γδ T cells and NK T cells). Along the same line, CD56 titration aims to position NK CD56+ cells between the CD3+ and the CD3 population.

  1. Maximum stain index curve
    NOTE:
    Titration of anti-CD3, -CD8, -CD14, -CD19, and -TCR γδ follows the standard procedure by which the concentration of antibody to optimally separate positive and negative peaks is derived by a maximum staining index curve. If antibodies against other markers are added to the panel, they also need to be titrated with a maximum staining index curve.
    1. Prepare a 2-fold antibody dilution by filling 10 wells of a 96-well plate with 40 µL of staining buffer. In the first well, increase the final volume to 80 µL of staining buffer and add the antibody of interest at a concentration 4 times the concentration suggested by the manufacturer.
    2. Mix well and transfer 40 µL to the second well. Mix well and repeat this step for all the other wells.
    3. Stain 10 samples of PBMC or whole blood with 30 µL of the 10 different 2-fold dilutions of antibodies following the protocol described before.
    4. Acquire data with a flow cytometer and plot the signal from each dilution (Figure 1A).
    5. Gate on the negative and positive populations for each antibody concentration. Increasing the concentration of antibodies can lead to a higher background. Therefore, resize the negative gate accordingly.
    6. For each antibody concentration, extract information about the median and standard deviation for the fluorescent intensity of the negative population, and the median for the fluorescent intensity of the positive population. Calculate for each antibody concentration the stain index with this formula: (median fluorescent intensity of the positive population — median fluorescent intensity of the negative population) ÷ (2 x standard deviation of the fluorescent intensity of the negative population) (Figure 1B).
    7. Plot the stain index vs. the antibody concentration expressed as a fraction of the antibody dilution (e.g., 1:10 dilution = 0.1), and identify the concentration of the antibody with the maximum stain index value (Figure 1C).
  2. Anti-CD4 and -CD56 antibody titration
    NOTE:
    Anti-CD4 and -CD56 antibody titration relies on the previous titration of the other markers in the two-fluorochrome panel. For the anti-CD4 antibody, the titration aims at placing the anti-CD4 signal between the double CD8+/CD3+ signal and the CD3 single positive population (Figure 1D).
    1. Titrate the anti-CD4 and CD56 antibodies with a 2-fold dilution strategy as described before, adding additional concentrations in between to finely identify the range of concentration that allows to separate CD4+ T cells and NK cells from the other cell populations.
    2. Titrate the anti-CD4 antibody by placing the anti-CD4 signal between the double CD8+/CD3+ signal and the CD3 single positive population (Figure 1D).
      NOTE: Special care should be done to clearly separate CD4+ T cells from CD8+ dim populations.
    3. Titrate the anti-CD56 antibody following a strategy similar to the anti-CD4 antibody titration, by placing NK cells between the CD3-negative and the CD3-positive populations.

3. Gating Strategy

  1. Identify lymphocytic and monocytic cell populations and remove dead cells and most of the residual red blood cells from the analysis.
    1. Select the entire population containing lymphocytes and monocytes based on forward vs side scatter area (FSC-A vs SSC-A). Remove cell aggregates from the analysis via forward scatter height vs forward scatter width (FSC-H vs FSC-W) and side scatter height vs side scatter width (SSC-H vs SSC-W).
    2. Use a live/dead discrimination marker to exclude bright positive dead cells and residual red blood cells from the analysis. Gate on lymphocytes and monocytes based on the different FSC-A and SSC-A profiles.
  2. Two-fluorochrome seven-marker gating strategy of the lymphocytic populations.
    NOTE: Within the CD3 positive subgroup, CD4+, CD8+, and γδ T cells can be separated using antibodies that solely target CD4, CD8, and the γδ receptor. In a comparable way, within the CD3 negative subgroup, B cells, NK cells, and monocytes can be uniquely identified using antibodies against CD19, CD56, and CD14, respectively.
    1. Select the lymphocyte gate and create a dot plot with on each axis one of two fluorochromes used in this protocol (Figure 2B).
    2. Gate on CD8+ T cells identified as CD3+/CD8+ double positive cells at the top right corner of the dot-plot (Figure 2B). Exclude the dim CD8 population which might contain NKT cells. Gate on CD4+ T cells identified as population in between CD8+ T cells and the CD3 single positive populations. Gate on γδ T cells identified as high CD3 cells. Subdivide γδ T cells in CD8 positive and CD8 negative.
    3. Gate on NK cells identified as the population in between CD3-positive and CD3-negative cells. Subdivide NK cells in CD8 positive and CD8 negative. Gate on B cells identified as CD3-negative CD19+ population on the right lower corner of the dot plot.
    4. Select the monocyte gates and create a dot plot with on each axis one of two fluorochromes used in this protocol (Figure 2C). Gate on the CD3/CD14+ population.

Table 1: Antibody panel used for the two-fluorochrome immune-cell staining of PBMC (BV421-PE combination).

Target Clone Fluorochrome Vendor Concentration Purpose
CD3 UCHT1 BV421 BD 1/20 Lineage
CD56 NCAM16.2 BV421 BD 1/900
TCRγδ B1 BV421 Bio 1/30
CD4 RPA-T4 PE BD 1/450
CD8 RPA-T8 PE BD 1/20
CD14 M5E2 PE BD 1/15
CD19 HIB19 PE BD 1/300
Dead cells L/D Blue LT 1/300 Live/Dead discrimination
BD = BD Biosciences, Bio = BioLegend, LT = Life Technologies

Table 2: Antibody panel used for the two-fluorochrome immune-cell staining of PBMC (APC-PE combination).

Target Clone Fluorochrome Vendor Concentration Purpose
CD3 UCHT1 APC BD 1/20 Lineage
CD56 NCAM16.2 APC BD 1/60
TCRγδ B1 APC Bio 1/30
CD4 RPA-T4 PE BD 1/450
CD8 RPA-T8 PE BD 1/20
CD14 M5E2 PE BD 1/15
CD19 HIB19 PE BD 1/300
Dead cells L/D Blue LT 1/300 Live/Dead discrimination
BD = BD Biosciences, Bio = BioLegend, LT = Life Technologies

Table 3: Antibody panel used to stain frozen PBMC from a patient with multiple myeloma.

Target Clone Fluorochrome Catalog Vendor Concentration Purpose
CD3 UCHT1 BV421 562426 BD 1/20 Lineage
CD56 NCAM16.2 BV421 562751 BD 1/900
TCRγδ B1 BV421 331217 Bio 1/30
CD4 RPA-T4 PE 555347 BD 1/450
CD8 RPA-T8 PE 555367 BD 1/20
CD14 M5E2 PE 555398 BD 1/15
CD19 HIB19 PE 555413 BD 1/300
CCR7 G043H7 AF647 353217 Bio 1/30 Differentiation
CD45RA HI100 APC-H7 560674 BD 1/60
CCR4 1G1 PE-Cy7 561034 BD 1/60 Th subsets
CCR6 G034-E3 BV605 353419 Bio 1/30
CXCR3 1C6/CXCR3 AF488 561730 BD 1/30
CD57 NK-1 PE-CF594 562488 BD 1/900 Activation/Exhaustion
HLA-DR G46-6 BV510 563083 BD 1/30
CD16 3G8 BUV395 563784 BD 1/30 NK, Monocyte activation
Dead cells L/D Blue L-23105 LT 1/300 Live/Dead discrimination

Representative Results

Figure 1
Figure 1: Representative antibody titration. (A) The dot plot shows CD8 expression on fresh PBMC stained with the indicated concentration of the antibody. (B) The table represents the median and standard deviation of fluorescent intensity of the CD8+, median fluorescent intensity CD8- population, and the derived stain index for each concentration tested. (C) The graph shows how to derivate the optimal concentration of the antibody as a function of stain index. (D) Representative titration of CD4 antibody. Panel D has been modified from Boin et al. 2017

Figure 2
Figure 2: Representative gating strategy and results of subpopulation discrimination. (A) Schematic representation of doublet exclusion, live cell discrimination, and size-based gating of lymphocytes and monocytes. (B) Lymphocyte subpopulations identified with the two fluorochrome approach. (C) Monocytes identified with the two fluorochrome approach. The figure has been modified from Boin et al. 2017

Divulgazioni

The authors have nothing to disclose.

Materials

CD3 BD Biosciences 562426 Antibody for staining
RRID: AB_11152082
CD56 BD Biosciences 562751 Antibody for staining
RRID: AB_2732054
TCRgd BD Biosciences 331217 Antibody for staining
RRID: AB_2562316
CD4 BD Biosciences 555347 Antibody for staining
RRID: AB_395752
CD8 BD Biosciences 555367 Antibody for staining
RRID: AB_395770
CD14 BD Biosciences 555398 Antibody for staining
RRID: AB_395799
CD19 BD Biosciences 555413 Antibody for staining
RRID: AB_395813
CD3 BD Biosciences 555335 Antibody for staining
RRID: AB_398591
CD56 BD Biosciences 555518 Antibody for staining
RRID: AB_398601
TCRgd BD Biosciences 331211 Antibody for staining
RRID: AB_1089215
CCR7 Biolegend 353217 Antibody for staining
RRID: AB_10913812
CD45RA BD Biosciences 560674 Antibody for staining
RRID: AB_1727497
CCR4 BD Biosciences 561034 Antibody for staining
RRID: AB_10563066
CCR6 BD Biosciences 353419 Antibody for staining
RRID: AB_11124539
CXCR3 BD Biosciences 561730 Antibody for staining
RRID: AB_10894207
CD57 BD Biosciences 562488 Antibody for staining
RRID: AB_2737625
HLA-DR BD Biosciences 563083 Antibody for staining
RRID: AB_2737994
CD16 BD Biosciences 563784 Antibody for staining
RRID: AB_2744293
Dead cells Life technologies L-23105 Live/dead discrimination
96-well V-bottom plate Thermo fisher 249570 plate for staining
FACSAria IIu Cell Sorter BD Biosciences Flow cytometer
FCS Express 6 De Novo Software FACS analysis
Graphpad Prism GraphPad software Data analysis

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Citazione di questo articolo
A Flow Cytometry Assay to Identify Immune Cell Subsets in Peripheral Blood Mononuclear Cells. J. Vis. Exp. (Pending Publication), e21987, doi: (2024).

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