Identification of Rare Antigen-Specific T Cells from Mouse Lungs with Peptide:Major Histocompatibility Complex Tetramers

Abstract

The identification and characterization of antigen-specific T cells during health and disease remains a key to improving our understanding of immune pathophysiology. The technical challenges of tracking antigen-specific T cell populations within the endogenous T cell repertoire have been greatly advanced by the development of peptide:MHC tetramer reagents. These fluorescently labeled soluble multimers of MHC class I or class II molecules complexed to antigenic peptide epitopes bind directly to T cells with corresponding T cell receptor (TCR) specificity and can, therefore, identify antigen-specific T cell populations in their native state without a requirement for a functional response induced by ex vivo stimulation. For exceedingly rare populations, tetramer-bound T cells can be magnetically enriched to increase the sensitivity and reliability of detection.

As the investigation of tissue-resident T cell immunity deepens, there is a pressing need to identify antigen-specific T cells that traffic to and reside in nonlymphoid tissues. In this protocol, we present a detailed set of instructions for the isolation and characterization of antigen-specific T cells present within mouse lungs. This involves the isolation of T cells from digested lung tissue followed by a general T cell magnetic enrichment step and tetramer staining for flow cytometry analysis and sorting. The steps highlighted in this protocol utilize common techniques and readily available reagents, making it accessible for nearly any researcher engaged in mouse T cell immunology, and are highly adaptable for a variety of downstream analyses of any low frequency antigen-specific T cell population residing within the lungs.

Introduction

At the heart of the adaptive immune system lies the ability of a T cell to recognize and respond to a specific antigen. When and where a T cell responds to its cognate antigen determines the balance of infection and autoimmunity, homeostasis and cancer, health and disease¹. It follows that the study of T cells in a specific context of immunity should focus on the cells with specificity for a relevant antigen of interest. Among the technological advancements that have greatly enhanced the ability to characterize antigen-specific T cell populations are fluorescently labeled soluble multimers (usually tetramers) of major histocompatibility complex (MHC) class I or class II molecules complexed to antigenic peptide epitopes, better known as "peptide:MHC tetramers"^2,3,4,5. By representing the natural ligands of T cell antigen receptors (TCRs), peptide:MHC class I and class II tetramers provide a means to directly identify antigen-specific CD8⁺ and CD4⁺ T cells, respectively, within the endogenous repertoire of T cells in the immune system without a requirement for a response to antigen stimulation in an assay. Tetramers represent a more elegant approach to the study of antigen-specific T cells than TCR transgenic T cell adoptive transfer models⁶, and have been increasingly used to identify foreign and self antigen-specific T cell populations in both experimental mouse models and human disease^4,5.

While tetramers can readily identify high-frequency populations of T cells that have expanded in response to antigen stimulation, their use for naive, self antigen-specific, or memory T cells is limited by the very low frequencies of these populations⁷. Our group and others have developed and popularized tetramer-based magnetic enrichment strategies that increase the sensitivity of detection to enable studies of these cell populations in mouse lymphoid tissues^8,9,10,11.

The emergence of tissue-resident T cells in the field has placed a heightened emphasis on developing new ways to investigate T cells in the nonlymphoid space. Like many other mucosal surfaces, T cells in the lungs encounter a range of self and foreign antigens derived from host epithelium, commensal and infectious microbes, and environmental entities, including allergens. Transcriptional analysis of T cells harvested from nonlymphoid tissue (NLT) demonstrates a memory-like phenotype that bears unique tissue-specific fate and function, often directed at trafficking and tissue homeostasis¹². Moreover, tissue-resident memory T cells (Trms) tend to be more clonally restricted than those in circulation¹³. Determining how and why antigens drive T cell residence in NLT is critical to understanding how the immune system protects against infection, maintains tissue homeostasis, and, at times, devolves into autoimmunity. However, there appears to be greater attrition amongst tissue-resident T cells from the lungs compared to other NLT¹⁴. Accordingly, the ability to identify and characterize endogenous T cells of the lung with a given antigen-specificity is limited by their inherent rarity.

By combining the use of magnetic bead-based cell enrichment techniques and peptide:MHC tetramer staining, we have succeeded in detecting expanded but rare self antigen-specific T cells in mouse lungs^15,16. Here, we present a detailed description of a protocol that we have optimized to reliably isolate and characterize any rare antigen-specific T cell population present in mouse lungs (Figure 1). This protocol incorporates an in vivo antibody staining step to distinguish tissue-resident from vascular T cells¹⁷ followed by two different methods for lung tissue processing to accommodate resource availability. This is then followed by a general T cell magnetic enrichment step, tetramer staining, and analysis by flow cytometry. Cell viability and tetramer staining is further enhanced in this protocol by the addition of aminoguanidine, which blocks inducible nitric oxide synthase (iNOS)-mediated T cell activation-induced apoptosis¹⁸ and Dasatinib which limits TCR downregulation¹⁹. The steps highlighted in this protocol utilize common techniques and readily available reagents, making it accessible for nearly any researcher engaged in mouse T cell immunology and is highly adaptable for a variety of downstream analyses. Although naive T cells are not likely to be found in the lungs, we believe this protocol will be particularly helpful for the study of self antigen-specific T cells and Trms in the lungs.

Figure 1: Overview of protocol workflow. Lungs are harvested from mice and dissociated into single cells. Samples are subsequently enriched for T cells prior to staining with peptide:MHC tetramers and fluorescently-labeled antibodies for flow cytometric analysis. Please click here to view a larger version of this figure.

Protocol

The procedures described in this protocol are approved and developed in accordance with the guidelines set forth by the Institutional Animal Care and Use Committee (IACUC) of Massachusetts General Hospital, an American Association for the Accreditation of Laboratory Animal Care (AAALAC)-accredited animal management program. Experiments were performed on 8-12-week-old male and female mice on a C57BL/6 genetic background bred and maintained in the MGH animal facility under specific pathogen-free conditions.

1. Preparing stock solutions

1. Prepare HEPES buffer by dissolving 10 mM HEPES, 5 mM KCl, 1.8 mM CaCl₂, 150 mM NaCl, and 1 mM MgCl₂, and adjust to pH 7.4.
2. Prepare 10x Liberase stock solution by dissolving 700 µg/mL of Liberase Thermolysin Medium (TM) (see Table of Materials) in Hank's Balanced Salt Solution with Ca⁺⁺ and Mg⁺⁺ (see Table of Materials).
3. Prepare 10x aminoguanidine stock solution by dissolving 100 mM Aminoguanidine Hemisulfate Salt (see Table of Materials) in Hank's Balanced Salt Solution with Ca⁺⁺ and Mg⁺⁺ (see Table of Materials).
4. Prepare complete Eagle's Ham's Amino Acids (EHAA) medium by mixing EHAA medium (see Table of Materials) with 10% fetal bovine serum (FBS), 100 U/mL penicillin/streptomycin, 50 µg/mL gentamycin, 2 mM L-glutamine, and 55 µM 2-mercaptoethanol.
   NOTE: Other common T cell media, such as RPMI or DMEM, may also be used.
5. Prepare sorter buffer by mixing 1x PBS with 2% FBS and 0.05% sodium azide.
6. Prepare Fc block by diluting purified anti-mouse CD16/32 antibody (see Table of Materials) at 1:100 v/v in sorter buffer.
7. Prepare Liberase TM/DNase digestion solution by adding 100 µg/mL Liberase TM and 50 µg/mL DNase I (see Table of Materials) in RPMI 1640 medium without L-glutamine (see Table of Materials).
8. Prepare ketamine/xylazine mixture by adding 10 mg/mL ketamine (see Table of Materials) and 1 mg/mL xylazine (see Table of Materials) in normal saline (0.9% NaCl) (see Table of Materials).

2. Generating single-cell suspension from lung tissue via automated tissue dissociator

1. For each mouse, prepare 4 mL of ice-cold HEPES buffer in a specialized tissue dissociator tube (see Table of Materials) and keep it on ice.
2. Anesthetize mice by intraperitoneal injection of 150-200 µL of ketamine/xylazine mixture. Inject 1-3 µg of fluorophore-conjugated anti-mouse CD45 antibody (see Table of Materials) diluted in 100 µL normal saline intravenously into each anesthetized mouse. Euthanize the mouse 3 min after antibody administration with an intraperitoneal injection of 500-600 µL of ketamine/xylazine mixture.
3. Resect the lungs and place them in their respective tissue dissociator tube chilled on ice. Place the tubes onto the automated tissue dissociator (see Table of Materials) and run the first program (preset program) for lung tissue.
4. Add 500 µL of Liberase stock solution and 500 µL of aminoguanidine stock solution to each tube containing the dissociated lung tissue. Incubate on a nutating mixer for 30 min at 37 °C.
5. Place the tubes back on the dissociator and run the second program (preset program) for lung tissue.
6. Pour the single-cell suspension from the tissue dissociator tube through a 100 µm cell strainer (see Table of Materials) into a 50 mL conical tube. Rinse the tissue dissociator tube with 5 mL of complete EHAA (or any equivalent T cell medium) and pass through the strainer into the 50 mL tube.
7. Remove the strainer and raise the volume of the cell suspension to 50 mL with complete EHAA. Centrifuge the cell suspension at 400 x g for 5 min at 4 °C. Carefully aspirate the supernatant, leaving behind approximately 100 µL of supernatant and cell pellet.
8. Add approximately 100 µL of Fc Block solution to bring the total volume up to 200 µL and vortex vigorously to resuspend the pellet.

3. Alternative protocol: Generating single-cell suspension from lung tissue via manual dissociation

1. For each mouse, prepare 1 mL of complete EHAA in a 1.5 mL microfuge tube and keep on ice.
2. Anesthetize mice by intraperitoneal injection of 150-200 µL of ketamine/xylazine mixture. Inject 1-3 µg of fluorophore-conjugated anti-mouse CD45 antibody diluted in 100 µL of normal saline intravenously into each anesthetized mouse. Euthanize the mouse 3 min after antibody administration with an intraperitoneal injection of 500-600 µL of ketamine/xylazine mixture.
3. Resect the lungs and place them in their respective 1.5 mL microfuge tube chilled on ice.
4. Once all the lungs have been harvested, transfer each lung to a fresh microfuge tube without any cell media.
5. Cut the lungs into small fragments (~2-3 mm chunks) using scissors within the microfuge tube.
6. Add 1 mL of Liberase TM/DNase I digestion cocktail to each tube.
7. Incubate for 30 min at 37 °C in a water bath. Return the samples to ice afterward to prevent over-digestion.
8. Pour the sample over a 100 µm cell strainer placed on top of a 50 mL conical tube. Mash the tissue against the mesh with the rubber end of the plunger from a sterile 1 mL syringe.
9. Rinse the strainer with cold sorter buffer, collecting a final volume of 7 mL in the tube. Centrifuge the cell suspension at 400 x g for 5 min at 4 °C. Carefully aspirate the supernatant, leaving approximately 100 µL of supernatant and cell pellet.
10. Add 100 µL of Fc Block solution to bring the total volume up to 200 µL and vortex vigorously to resuspend the pellet.

4. Enriching the lung sample for T cells via magnetic bead enrichment

1. Add 50 µL of anti-mouse CD90.2 microbeads (see Table of Materials). Vortex and incubate for 10 min at 4 °C.
   NOTE: CD90.2 corresponds to the allele expressed by T cells in C57BL/6 mice. Check allele genotype if other strains of mice are used.
2. In the meantime, place a paramagnetic cell separation column (see Table of Materials) onto a one or four position cell separation magnet (see Table of Materials). Position an open 15 mL conical tube under each column to capture the flow through. Prime the column with 3 mL of cold sorter buffer, allowing the column to drain by gravity into the conical tube below.
3. Once the cells have incubated with the microbeads for 10 min, add cold sorter buffer to a volume of 1 mL and transfer through a 100 µm cell strainer placed atop the column. Collect the column flow through into a fresh 15 mL conical tube placed below the column.
4. Once the cell suspension has completely drained through the column by gravity, wash the column by rinsing the original tube with an additional 3 mL of cold sorter buffer and applying it to the column through the mesh, thereby rinsing the strainer. Remove the strainer.
5. When the sample has again completely drained into the column, and no further flowthrough is exiting the column, remove the column from the magnet and place it atop a fresh 15 mL conical tube.
6. Add 5 mL of cold sorter buffer to the column.
7. Immediately elute the cells bound to the column by pushing the column plunger into the top in one continuous motion and forcing the sorter buffer out of the bottom of the column into the new tube.
8. Centrifuge the eluted samples at 400 x g for 5 min at 4 °C. Carefully aspirate the supernatant, leaving behind approximately 100 µL of supernatant and cell pellet.
9. Add 100 µL of cold sorter buffer to bring the total volume up to 200 µL and vortex vigorously to resuspend the pellet.
10. Analyze the flowthrough sample containing the unbound cell fraction, if desired.

5. Staining the antigen-specific T cells with peptide:MHC tetramers

1. Add 1 µL of 10 µM Dasatinib (see Table of Materials) to each sample, vortex, and incubate for 5 min at RT.
2. Add PE- or APC-conjugated peptide:MHC tetramer to a final concentration of 10 nM (or empirically optimized concentration for a given tetramer).
3. Vortex and incubate in the dark for 1 h at RT (or empirically optimized time and temperature).

6. Analyzing the tetramer-labeled T cells by flow cytometry

1. While the sample is being stained with peptide:MHC tetramers, prepare a master mix of antibodies to stain the surface markers of the cells (Table 1).
   ​NOTE: Avoid fluorophores that conflict with the intravenously administered CD45 antibody or the tetramers.
2. With 15 min left in the incubation period for tetramer-staining, add surface antibody master mix at 1:100 (or empirically optimized concentration) to each sample.
3. Continue to incubate in the dark at RT for the remainder of the 1 h incubation period.
4. Add 50,000 flow cytometry count beads (see Table of Materials) and add cold sorter buffer to a final volume of approximately 5 mL. Centrifuge the stained sample at 400 x g for 5 min at 4 °C. Carefully aspirate the supernatant, leaving behind approximately 100 µL of supernatant and cell/bead pellet.
5. Resuspend the sample with an additional 200 µL of sorter buffer and transfer the sample to a 5 mL fluorescence activated cell sorting (FACS) tube.
6. Analyze the sample on a flow cytometer. Collect as many cells as possible, up to a maximum of 2,500,000 total events. Ensure that at least 20,000 count bead events have been collected. Keep the acquisition rate at or below 5,000 events per second.
7. Save all data as FCS files.

  

Fluorochrome	Antibody
BUV395	CD90.2
Pacific Blue	CD45 (added earlier by i.v. injection)
Pacific Orange	CD8
Brilliant Violet 785	CD4
FITC	CD3
PerCP-Cy5.5	Dump (B220, CD11b, CD11c, F4/80)
PE	pMHC tetramer or phenotypic marker
PE-Cy7	Phenotypic marker (e.g. CD44, PD-1, CD69, etc.)
APC	pMHC tetramer or phenotypic marker
AlexaFluor 700	Phenotypic marker (e.g. CD44, PD-1, CD69, etc.)
APC-Cy7	Live/dead stain

Table 1: Sample staining matrix. A typical panel of fluorophore-conjugated flow cytometry antibodies utilized for identifying and characterizing antigen-specific T cells.

7. Analyzing data

1. Analyze the FCS data files using appropriate flow cytometry software.
   1. Set up a sequence of successive inclusion gates to identify 1) lymphocyte-like, 2) single, 3) live, 4) extravascular, 5) dump-negative, and 6) CD90.2-positive events that are either CD4 or CD8 positive (Figure 2).
   2. Identify the tetramer-positive T cells within these populations.
2. Determine absolute tetramer-positive cell counts by calculating the ratio of beads added (50,000) to the number of beads collected during the sample run and multiplying the value with the total number of tetramer-positive cells collected.
   

Representative Results

Figure 2 depicts the representative gating strategy used in the identification of rare antigen-specific CD4⁺ T cells in the lungs with peptide:MHC class II tetramers. The same process can be applied for antigen-specific CD8⁺ T cells with peptide:MHC class I tetramers (data not shown).

Due to the high number of nonlymphoid cells in the lungs, the reliable detection of rare antigen-specific T cells by tetramer requires some form of prior enrichment for the T cells of interest to improve signal-to-noise. Figure 3 illustrates the efficacy of the CD90.2 antibody-based magnetic enrichment of total T cells from lung tissue that we have described in this protocol. On average, we recover greater than 99% of all CD90.2⁺ T cells from the lungs with greater than 90% purity via this enrichment process. Figure 4 illustrates the improved detection of rare tetramer-positive CD4⁺ T cells resulting from this enrichment versus no enrichment or a direct tetramer-based cell enrichment strategy.

Figure 5 illustrates the improved tetramer-labeling of antigen-specific T cells treated with Dasatinib, particularly in rare populations.

Figure 2: Gating strategy for flow cytometry analysis. Sequential inclusion and exclusion gates used to identify rare self antigen-specific CD4+ T cells that accumulate in the lungs following acute tissue injury. Count beads can be identified directly based on their fluorescence along the FITC channel. Please click here to view a larger version of this figure.

Figure 3: CD90.2 antibody-based magnetic enrichment of total T cells in the lungs. Representative flow cytometry plots are shown for the unbound (left) and bound (right) fractions of a lung sample following enrichment. Please click here to view a larger version of this figure.

Figure 4: Comparison of cell enrichment strategies to aid detection of rare antigen-specific T cells in the lungs. Three mice expressing a model self antigen in lung epithelium were immunized subcutaneously with a peptide epitope from the self antigen emulsified in Complete Freund's Adjuvant (CFA). After 7 days, mouse lungs were harvested, combined, and split into three equal samples for tetramer-staining following no cell enrichment (left), CD90.2 antibody-based cell enrichment (center), or tetramer-based cell enrichment (right). Samples were analyzed by flow cytometry for no more than 1,500,000 total events (CD4⁺ gated events shown). Numbers of tetramer-positive events are noted in black, while the computed total numbers of antigen-specific T cells in the lung samples are indicated in red. Please click here to view a larger version of this figure.

Figure 5: Dasatinib treatment enhances tetramer-staining. Wildtype mice (left) or mice expressing a model self antigen in lung epithelium (right) were immunized subcutaneously with a peptide epitope from the self-antigen emulsified in CFA. The spleens and lymphoid organs from the mice were harvested, combined, and split into two equal samples for labeling with peptide:MHC class II tetramers with or without dasatinib pre-treatment. Histograms of tetramer-staining are overlaid, comparing samples treated with (red) and without (blue) dasatinib. The median fluorescence intensity of each sample is indicated. Please click here to view a larger version of this figure.

Discussion

Prior characterizations of antigen-specific T cells from the lungs have benefitted from the robust numbers of antigen-specific T cells that expand following an acute priming event such as intranasal immunization or infection^20,21,22. However, rarer T cell populations in the lungs, such as self antigen-specific T cells or tissue-resident memory T cells, are difficult to detect without some form of sample enrichment for the T cells of interest^15,16,23. We have achieved this goal by combining lung tissue dissociation techniques previously described to yield a high percentage of viable lymphocytes^24,25 with a strategy to discriminate intravascular from parenchymal T cells and a general T cell-based enrichment process followed by tetramer staining¹⁷. Using this protocol, we have demonstrated the ability to identify and characterize rare T cells that are specific against self antigens in the lung that arise in response to direct immunization with exogenous peptide or indirect activation from antigen release during tissue damage^15,16. Several considerations were made in the development of this protocol.

We have described two different lung tissue processing protocols that have worked well. One involves the use of an automated tissue dissociation instrument, while the other relies on a manual process. Importantly, both methods utilize Liberase TM, a blend of collagenase I and II which also contains a metalloprotease thermolysin. This enzyme blend has been demonstrated to increase digestive activity over a single collagenase cocktail and has been demonstrated to work well with the recovery of leukocytes from lung tissue²⁶.

The automated tissue dissociation protocol requires a large upfront cost for the machine and specialized tissue dissociation tubes, but the tubes can be washed and reused along with cell strainers, which are also generally reusable. The manual dissociation protocol does not incur the upfront cost of specialized equipment, but it is labor-intensive and prolongs the harvest as each sample is chopped up individually. There are other differences between the protocols regarding the use of aminoguanidine or DNase I to limit cell death and cell clumping, but we have not carefully compared the impact of these additives. The decision to use either protocol should depend on personal experience in the type of study being performed as well as the availability of an automated tissue dissociation instrument, which would represent the biggest factor in cost. Indeed, elements of the two protocols can be mixed and matched to provide the best performance for the specific needs of the study.

The protocol mentioned above notably excludes the use of a density gradient to isolate lymphocytes from the single-cell suspension prepared from tissue dissociation. We have found that the magnetic T cell enrichment step needed for the identification of rare antigen-specific T cells obviates this step. However, in cases where antigen-specific T cell frequencies are high enough to eliminate the need for a T cell enrichment step altogether, a density gradient is recommended as it will provide a substantial amount of target cell enrichment by removing a large number of nonlymphoid cells. Additionally, if the lung single-cell preparations are particularly large and/or messy, a density gradient step may be used prior to magnetic enrichment to remove excessive cell debris that might later clog the columns (steps 4.4-4.7).

We opted for a general enrichment of all T cells based on the CD90 pan T cell marker (CD90.2 for the allele expressed in C57BL/6 mice) instead of a more direct tetramer-based cell enrichment strategy. This offers several advantages. (1) CD90-based enrichment results in higher numbers of antigen-specific events detected on flow cytometry than either unenriched or tetramer-based enrichment samples (Figure 4). This contributes to better estimates of rare antigen-specific T cell frequencies without necessitating the collection of excessive numbers of total events (>2,500,000), which prolongs sample collection times and worsens signal-to-noise resolution. (2) Unlike tetramer-based enrichment, CD90-based enrichment allows for evaluation of the entire T cell compartment of the lung, including CD4⁺ and CD8⁺ T cells, intravascular vs. extravascular T cells, and antigen-specific vs. antigen-non-specific, all in one sample (Figure 2). (3) Because the CD90-based enrichment step occurs prior to tetramer staining, it minimizes the time before tetramer-labeled cells are analyzed on the flow cytometer, thereby limiting the potential loss of signal from tetramer detachment.

The T cell enrichment process in this protocol is based on positive selection with CD90.2 magnetic beads, but similar results can be achieved with negative selection strategies provided by CD4, CD8, or pan T cell isolation kits. We describe the use of a specific brand of microbeads, columns, and magnets, but other magnetic enrichment systems should work, too. Again, decisions should be based on performance in the specific study being performed as well as overall costs, which can be substantial. In our experience with enrichment protocols, there is a general tradeoff between target cell yield and purity, and for the purposes of detecting extremely limited numbers of antigen-specific T cells, yield takes precedence.

While the representative results depict experiments involving CD4⁺ T cells and peptide:MHC class II tetramers, this protocol is just as effective for CD8⁺ T cells and peptide:MHC class I tetramers. In such cases, considerations should be made for the potentially different conditions required by class I tetramer staining (concentration, time, temperature). Moreover, we do not see any reasons precluding its use for antigen-specific B cell studies with appropriate fluorochrome-labeled B cell antigen reagents²⁷.

Lastly, the protocol described here includes the addition of the protein kinase inhibitor Dasatinib to the sample prior to tetramer staining. Dasatinib blocks TCR signaling and internalization, which improves tetramer-labeling of T cells while also potentially reducing tetramer-induced T cell death¹⁹. We found the benefit of Dasatinib treatment most prominently in the detection of the rarer self antigen-specific population. This is likely due to the fact that self antigen-specific T cells express lower affinity TCR due to the effects of negative selection during central tolerance^28,29,30,31.

The protocol used here has been successfully combined with intracellular staining protocols to analyze transcription factor and cytokine expression in rare lung-resident antigen-specific T cells. We have also successfully flow-sorted these rare populations for downstream analyses, including single-cell transcriptomics and TCR sequencing. The continued use and development of this protocol should greatly benefit studies of adaptive immunity in lung pathophysiology.

Materials

Name	Company	Catalog Number	Comments
100 mm cell strainer	Fisher Scientific	22-363-549
10x PBS without Ca++ or Mg++	Corning	46-013-CM
1x PBS without Ca++ or Mg++	Corning	21-031-CV
AccuCheck Counting Beads	Invitrogen	PCB100
Aminoguanidine Hemisulfate Salt	Sigma-Aldrich	A7009
CD90.2 microbeads, mouse	Miltenyi	130-121-278
Cell separation magnet (MidiMACS Separator)	Miltenyi	130-042-302	Holds single LS column
Cell separation magnet (QuadroMACS Separator)	Miltenyi	130-090-976	Holds 4 LS columns
Dasatinib	Sigma-Aldrich	CDS023389
DNase I	Roche	10104159001
Eagle’s Ham’s Amino Acids medium	Sigma-Aldrich	C5572
gentleMACS	Miltenyi	130-093-235	Automated tissue dissociator
gentleMACS C Tubes	Miltenyi	130-093-237	Automated tissue dissociator tubes
Hank's Balanced Salt Solution with Ca++ or Mg++	Corning	21-020-CM
HEPES	Gibco	15630080
Ketamine	Vedco	NDC 50989-996-06
Liberase TM	Roche	5401119001
Pacific Blue anti-mouse CD45 antibody (Clone: 30-F11)	Biolegend	103126
Paramagnetic cell separation columns (LS Columns)	Miltenyi	130-042-401	Comes with plunger
Purified anti mouse CD16/32 antibody (Clone: 93)	Biolegend	101302
RPMI 1640 medium without L-glutamine	Corning	15-040-CM
Sodium Chloride 0.9% (Normal Saline)	Cytiva	Z1376
Xylazine	Pivetal	NDC 466066-750-02