USF Health

 
      


Cell Surface Staining

FACS Staining Method for Cell Surface Proteins

Staining medium (SM) (recipe below)

Sterile filtered calf serum (CS) 

1X Gey's solution (recipe below)

0.1% Trypan Blue

1 mg/ml propidium iodide (PI) [in ddH2O] (store frozen in 50 ml aliquots - can thaw & refreeze many times)

Nitex mesh, 85- µm mesh size

4 ml conical tubes [Diamed STK 8550]

5 ml round bottom tubes [Falcon 2052]

Antibodies as required for experiment


Sample Note:

For each FACS sample use 0.5-2x106 cells/tube. Up to 4x106 cells/sample can be used in a 50 µl staining volume, especially if analyzing rare cell populations. If larger cell numbers are stained, see Note (c) below. For peripheral blood lymphocytes (PBLs) use 1-8 X 105 cells/tube ie. whatever you can get.


Protocol:

Prepare antibody dilutions in SM based on a total staining volume of 50 µl diluted Ab per sample tube. Calculate total volume of antibody solution needed based on number of samples plus one for each stain.

Note that before using an antibody in an experiment, the optimal antibody concentration for your application should be determined by staining a test cell sample with serial dilutions of the antibody. See Note (e) below.


(a) For ex vivo cells, dissect desired tissue (usually lymphoid tissue) from animal and place on ice in a tissue culture dish with ice-cold SM.


(b) Make single cell suspension. Place tissue on pre-wet steel mesh screen that is sitting in a 35-mm tissue culture dish. Mince tissue with scissors and push through steel screen using the plunger from a 3 ml syringe. Wash remaining cells through screen with ice-cold SM. Transfer cell suspension from tissue culture dish to a 15-ml Falcon 2096 tube on ice. Keep cells on ice throughout procedure.


 

For cultured cells, collect cells by decanting media and cells into a 15-ml Falcon 2096 or 50-ml Falcon 2070 tube. Keep cells on ice throughout procedure.


 

Exceptions apply for certain cultured cell lines. e.g. 293T cells should be kept at room temperature as they tend to die with prolonged incubation on ice. Centrifugation, counting and staining of these cells should be done at room temperature. Staining times should be kept to a minimum to avoid changes in observed phenotype due to metabolism during staining.


 

Underlay cell suspension with 0.5 ml CS. Collect cells by centrifugation at 400xg for 5 minutes at 4°C (1500 rpm in Beckmann GS6-KR).

 

The calf serum underlay helps make a more compact cell pellet and gets rid of some dead cells and cellular debris.

Aspirate supernatant.


Optional step:

Lyse red blood cells by re-suspending cell pellet in 1X Gey's solution. Incubate at room temperature 2-5 minutes. Add 10 ml SM, mix well and filter through Nitex. Underlay with 1-2 ml calf serum.


 

Incubation longer than 5 minutes should be avoided as this will lead to lysis of nucleated cells. Gey's solution should be used at a concentration of approximately 2x107 cells/ml. For one mouse spleen, resuspend pellet in 4-5 ml Gey's solution. For the bone marrow from one mouse, resuspend cell pellet in 2 ml Gey's solution. Thymocytes and lymph node cells do not need to be lysed, if tissues have been dissected properly. Thymocytes are sensitive cells, avoid lysis step if possible.


 

Collect all cells by centrifugation at 400 x g for 5 minutes at 4°C. Aspirate supernatant.

Re-suspend cell pellets in appropriate volume of SM (try to approximate a final concentration of 1-5x107/ml).

 

Count live cells by trypan blue exclusion in 0.1% Trypan blue on a hemacytometer.

Aliquot appropriate number of cells (see Sample Note above) into pre-labeled 4 ml FACS staining conical tubes. Add 0.5 ml of SM to each tube and underlay with 0.3 ml CS. Collect cells by centrifugation at 400xg for 5 minutes at 4°C.

 

The calf serum underlay helps make a more compact cell pellet, gets rid of some dead cells and cellular debris, makes the supernatant easier to aspirate without loss of cells, and also leaves less residual fluid behind that can further dilute the antibody solution.


Completely aspirate supernatant. Resuspend cell pellet in 50 µL 1° Ab stain in each tube. Incubate for 20-40 minutes on ice. Protect from light if fluorochrome-labeled 1° antibodies are being used.

 

Residual fluid can further dilute the antibody solution and adversely affect your staining results

 

Add 0.5 ml SM to each tube (i.e. 10 staining volumes) and underlay with 0.3 ml of CS using 5 ¾" pasteur pipettes.

 

Collect cells by centrifugation at 400xg for 5 minutes at 4°C.


Completely aspirate supernatant. Resuspend cell pellet in 50 µl 2° antibody. Protect from light. Incubate for 20-25 minutes on ice. If biotinylated 1° antibodies were used, incubate avidin-fluorochrome conjugate 2° stage for 30 minutes on ice.

 

Residual fluid can further dilute the antibody solution and adversely affect your staining results

 

Repeat wash steps 13 & 14.

 

Aspirate supernatant. Resuspend cell pellet in 0.5 ml of SM containing 1 µg/ml PI. Filter through Nitex screens (to remove clumps and debris) into labeled 5 ml round-bottom FACS tubes (Falcon 2052).

 

Collect data on flow cytometer. If this step is to be delayed more than 2-3 hours after staining is complete, they can be fixed in 1.6-4% paraformaldehyde and stored at 4°C overnight or for a few days. However, be sure to use SM without PI in Step 17. (See the related protocol "Fixing Stained Cells").


Buffers Staining Media (SM)

1X HBSS with Ca2+/Mg2+; 2% calf serum; 10mM HEPES, pH 7.2; 10 mM NaN3 (to prevent microbial growth). For some cell types it may be preferable to use HBSS without Ca2+/Mg2+. Store at 4°C.


Gey's Solution

Stock A: 35.0 g NH4Cl; 1.85 g KCl; 1.13 g Na2HPO4• 7H2O; 0.12 g KH2PO4; 5.0 g glucose
Bring to 1 L with ddH2O and autoclave.

Stock B: 0.42 g MgCl2•6H2O; 0.14 g MgSO4•7H2O; 0.34 g CaCl2
Bring to 100 ml with ddH2O and autoclave.

Stock C: 2.25 g NaHCO3
Bring to 100 ml with ddH2O and autoclave.


1X Gey's Solution:
20 parts Stock A; 5 parts Stock B, 5 parts Stock C; 70 parts sterile ddH2O. If not prepared aseptically, add 10 mM NaN3 (to prevent microbial growth). Store at 4°C.


0.1% Trypan Blue

Dilute 0.4% Trypan blue (Sigma, T-8154) 1:4 in 1X PBS, pH 7.2, with 5mM NaN3. Filter through a 0.2 µm filter.


Notes

If using NaN3 in SM, make sure to keep cells cold as the azide kills cells at room temperature.

 

If cells are being used in subsequent in vivo or in vitro assays, leave out the azide, filter sterilize all solutions and handle cells aseptically. Nitex can be autoclaved in sealed pouches. Alternatively, sterile cell strainers (Falcon #2350; 70µm mesh) can be used if dealing with limited sample numbers.

 

To scale up staining, keep cells at 4-10 x 107cells/ml. Wash with 5-10x staining volume, and underlay with 0.5-l mL CS. After last wash, filter through nylon mesh and adjust cell density to 1-10 x 106cells/mL in SM with PI.

 

If you are troubled by high levels of non-specific background staining, try removing antibody aggregates: airfuge reagents (concentrated unconjugated, FITC, TR, or biotin conjugates) for 10 min. For APC/PE conjugates → microfuge for 10 min in cold room. Always keep Ab stocks on ice and in the dark if using directly conjugated preps.

For each 1° or 2° Ab, the saturating concentration must be determined empirically. A 3-fold diltution series is often most useful (eg. 1/50, 1/150, 1/450, etc.) with appropriate cells. Antibody vendors often recommend a concentration to use, but in our experience these are usually excessive and often not optimal. Depending on cell frequency and antigen expression levels, different tissues may require different antibody concentrations. Staining should always be done with Ab at 2X saturation. For further information, consult our Antibody Titration Protocol.

 

References:

1. Holmes, K., Lantz, L.M., Fowlkes, B.J., Schmid, I., and Giorgi, J.V. (2001) Preparation of Cells and Reagents for Flow Cytometry. Coligan et al. (Eds.) In Current Protocols in Immunology, pp. 5.3.1-5.3.24. John Wiley & Sons, Inc.


2. Strober, W. (1997). Common Immunologic Techniques - Monitoring Cell Growth. Coligan et al. (Eds.) In Current Protocols in Immunology, pp. A.3A.1-A.3A.2. John Wiley & Sons, Inc.

 

Fixing Stained Cells for Subsequent Flow Cytometric Analysis

BD Biosciences and Alternate Protocol

 

Materials

Staining medium (SM) [1X HBSS; 2% (v/v) calf serum; 10mM NaN3, 10 mM HEPES [pH 7.2]

1X PBS

BD Cytofix (contains 4% paraformadehyde), Cat # 554655

OR

Paraformaldehyde solution, 16%, Canemco Inc, Cat #017B

Filtered calf serum (CS) [0.45 m TC sterile filtered to avoid bacterial growth]

0.1% Trypan Blue

Nitex mesh, 85-µm mesh size

4 ml conical tubes [Diamed STK 8550]

5 ml round bottom tubes [Falcon 2052]


Sample Note:

For each FACS sample use 0.5-2x106 cells/tube. A considerable amount of cell loss will occur during the multiple washes and spins. The CS is used to underlay the cell suspension during washes. DO NOT add PI to the SM used in step 5 (BD protocol) or step 6 (alternate protocol), because the cells are now permeabilized and will all be PI positive.

 

BD Cytofix Protocol:

Perform staining for extracellular markers according to any other standard FACS staining protocol.

 

Wash cells by adding 500-1000µl SM, underlay with 250-300 l CS and collect by centrifugation at 400xg for 5 minutes at 4°C (1500 rpm in Beckmann GS6-KR). Aspirate supernatant.

 

Fix cells by re-suspending cell pellet in 200µl of BD Cytofix Buffer™ per tube. Incubate cells for 20-30 minutes on ice. (Note: Cell aggregation can be avoided by briefly vortexing cells prior to addition of the fixation buffer).

 

Wash cells by adding 500-1000µl SM (omit the CS underlay at this point because of the fixative in the buffer) and collect by centrifugation as described above. Aspirate supernatant.

 

Re-suspend cells in 500µl SM, filter through Nitex mesh and store at 4°C, protected from light until ready to run samples on the cytometer.


Alternative Protocol:

Perform staining for extracellular markers according to any other standard FACS staining protocol.

 

Wash cells in SM by adding 500-1000µl SM, underlay with 250-300µl CS and collect by centrifugation as described above. Aspirate supernatant.

 

In the meantime, prepare 2% paraformaldehyde solution in 1xPBS (from16% paraformaldehyde stock). This working solution is stable for a week when stored at 4°C, in an airtight container, protected from light, provided that the solution remains at pH 7.

Fix cells by re-suspending the pellet in 500-1000µl of 2% paraformaldehyde. Alternatively, clumping may be best avoided first resuspending cells in 900µl 1xPBS and then adding 100µl 16% parafromaldehyde for a final concentration of 1.6%. Incubate at room temperature for 10 minutes or for 20-30 minutes on ice.

 

Wash cells in 2ml of 1xHBSS or 1xPBS SM (omit the CS underlay at this point because of the fixative in the buffer) and collect by centrifugation. Aspirate supernatant.

Re-suspend cells in 500 lµSM, filter through Nitex mesh and store at 4°C, protected from light until ready to run samples on the cytometer.


Note:
works well with all fluorochromes, including PE and APC based tandem conjugates. It is recommended that fixed samples be run on the cytometer within 1 week, preferably the next day. Autofluorescence tends to increase and sample quality generally declines with long-term storage of fixed samples.