Assessment of Cellular Bioenergetics in Mouse Hematopoietic Stem and Primitive Progenitor Cells using the Extracellular Flux Analyzer

Summary

The method presented here summarizes optimized protocols for assessing cellular bioenergetics in non-adherent mouse hematopoietic stem and primitive progenitor cells (HSPCs) using the extracellular flux analyzer to measure the extracellular acidification rate (ECAR) and oxygen consumption rate (OCR) of HSPCs in real time.

Abstract

Under steady state, hematopoietic stem cells (HSCs) remain largely quiescent and are believed to be predominantly reliant on glycolysis to meet their energetic needs. However, under stress conditions such as infection or blood loss, HSCs become proliferative and rapidly produce downstream progenitor cells, which in turn further differentiate, ultimately producing mature blood cells. During this transition and differentiation process, HSCs exit from quiescence and rapidly undergo a metabolic switch from glycolysis to oxidative phosphorylation (OxPHOS). Various stress conditions, such as aging, cancer, diabetes, and obesity, can negatively impact mitochondrial function and thus can alter the metabolic reprogramming and differentiation of HSCs and progenitors during hematopoiesis. Valuable insights into glycolytic and mitochondrial functions of HSCs and progenitors under normal and stress conditions can be gained through the assessment of their extracellular acidification rate (ECAR) and oxygen consumption rate (OCR), which are indicators of cellular glycolysis and mitochondrial respiration, respectively.

Here, a detailed protocol is provided to measure ECAR and OCR in mouse bone marrow-derived lineage-negative cell populations, which include both hematopoietic stem and primitive progenitor cells (HSPCs), using the extracellular flux analyzer. This protocol describes approaches to isolate lineage-negative cells from mouse bone marrow, explains optimization of cell seeding density and concentrations of 2-deoxy-D-glucose (2-DG, a glucose analog that inhibits glycolysis) and various OxPHOS-targeted drugs (oligomycin, FCCP, rotenone, and antimycin A) used in these assays, and describes drug treatment strategies. Key parameters of glycolytic flux, such as glycolysis, glycolytic capacity, and glycolytic reserve, and OxPHOS parameters, such as basal respiration, maximal respiration, proton leak, ATP production, spare respiratory capacity, and coupling efficiency, can be measured in these assays. This protocol allows ECAR and OCR measurements on non-adherent HSPCs and can be generalized to optimize analysis conditions for any type of suspension cells.

Introduction

Hematopoiesis is the process by which various types of mature blood cells with highly specialized functions are formed from HSCs¹. HSCs are capable of self-renewal and differentiation into various multipotent and lineage-specific progenitor populations. These progenitors ultimately produce cells of lymphoid, myeloid, erythroid, and megakaryocyte lineages. To maintain their self-renewal capacity, HSCs remain largely quiescent and, like other tissue stem cells, are believed to rely on glycolysis rather than mitochondrial OxPHOS for ATP production^2,3. Entry into the cell cycle leads to enhanced respiration and OxPHOS, resulting in elevated levels of reactive oxygen species (ROS), which are detrimental to HSC maintenance and function³. Repeated cell division thus may lead to reduced self-renewal capacity of HSCs and ultimately to their exhaustion.

In adult hematopoiesis, HSCs primarily undergo asymmetric cell division, during which one of the daughter cells retains HSC potential and continues to rely on glycolytic metabolism. The other daughter cell becomes a primitive progenitor cell that loses self-renewal capacity but proliferates and eventually gives rise to differentiated functional hematopoietic cells⁴. When HSCs differentiate to produce downstream progenitors, a switch from glycolysis to mitochondrial metabolism is thought to occur to supply the energy and building blocks needed to support this rapid transition⁵, as suggested by the observations that HSCs possess inactive mitochondrial mass^6,7,8,9. In contrast, mitochondrial activity (indicated by linked ROS levels) is much higher in lineage-committed progenitors than in HSCs^9,10,11. Metabolic changes that occur during the earliest step of hematopoiesis thus suggest a direct and crucial role of mitochondria in regulating HSC fate.

Dysfunctional mitochondria present under various stress conditions, such as aging, cancer, diabetes, and obesity¹², can interfere with HSC self-renewal capacity, inducing an imbalance in HSC/progenitor differentiation by producing excessive amounts of ROS, impairing ATP production, and/or by altering other metabolic processes^9,12,13. Perturbations in metabolic homeostasis in HSC/progenitor differentiation could significantly impact hematopoiesis, potentially contributing to the development of hematologic abnormalities¹³. Given the critical influences of glycolysis and mitochondrial OxPHOS on HSC stemness and differentiation, it is of interest to investigate both metabolic parameters under normal and stress conditions. Valuable insights into the glycolytic and mitochondrial function of HSCs and progenitor cells can be gained by assessing their ECAR and OCR, which are indicators of cellular glycolysis and mitochondrial respiration, respectively.

The Seahorse extracellular flux analyzer is a powerful apparatus equipped with two probes per well to simultaneously measure ECAR and OCR in live cells and thus can be used to assess cellular bioenergetics in real time, in response to various substrates or inhibitors. The assay cartridge used with the analyzer contains injection ports to hold up to four drugs for automated injection during the assay. A scheme of a typical glycolysis stress test is shown in Figure 1A. The assay starts with the measurement of ECAR of cells, incubated in glycolysis stress test medium containing glutamine but not glucose or pyruvate. This represents acidification occurring due to non-glycolytic activities of the cells and is reported as non-glycolytic acidification. This is followed by the injection of glucose at a saturating concentration. Via glycolysis, glucose in the cell is converted into pyruvate, which is further metabolized in the cytoplasm to produce lactate, or in mitochondria to produce CO₂ and water.

Conversion of glucose to lactate causes net production and subsequent release of protons into the extracellular medium, resulting in a rapid increase in the ECAR^14,15,16. This glucose-stimulated change in ECAR is reported as glycolysis under basal conditions. The second injection consists of oligomycin (an inhibitor of ATP synthase, a.k.a. complex V¹⁷), which inhibits mitochondrial ATP production. During oligomycin-mediated OxPHOS inhibition, cells maximally upregulate glycolysis to meet their energetic demands. This causes a further increase in ECAR, revealing the maximum glycolytic capacity of the cells. The difference between the maximum glycolytic capacity and basal glycolysis is referred to as glycolytic reserve. Finally, 2-DG is injected, which causes a significant drop in ECAR, usually close to non-glycolytic acidification levels. 2-DG is a glucose analog that competitively binds to hexokinase, resulting in inhibition of glycolysis¹⁸. Thus, the 2-DG-induced decrease in ECAR further confirms that glycolysis is indeed the source of ECAR observed after glucose and oligomycin injections.

Figure 1B displays the schematic for a typical mitochondrial stress test. The assay starts with baseline OCR measurement of the cells, incubated in mitochondrial stress test medium containing glucose, glutamine, and pyruvate. Following basal OCR measurements, oligomycin is injected in this assay, which inhibits complex V, thereby reducing electron flow through the electron transport chain (ETC)¹⁷. Consequently, OCR is reduced in response to oligomycin injection, and this decrease in OCR is linked to mitochondrial ATP production. The second injection consists of carbonyl cyanide-4 (trifluoromethoxy) phenylhydrazone (FCCP), a protonophore and an uncoupler of mitochondrial OxPHOS¹⁷. FCCP collapses the mitochondrial proton gradient by allowing the flow of protons across the mitochondrial inner membrane. Because of the FCCP injection, electron flow through the ETC is derepressed, and complex IV consumes oxygen at the maximal level. The difference between maximal OCR and basal OCR is referred to as the spare respiratory capacity, which is a measure of the cell's ability to respond to increased energy demand under stress conditions. Finally, a mixture of two ETC inhibitors (rotenone, a complex I inhibitor, and antimycin A, a complex III inhibitor¹⁷) is injected, which completely shuts down electron flow, and OCR decreases to a low level. OCR measured after rotenone and antimycin A injection corresponds to non-mitochondrial OCR driven by other processes inside the cells. Non-mitochondrial OCR enables the calculation of basal respiration, proton leak, and maximal respiration.

Basal respiration represents the difference between baseline OCR and non-mitochondrial OCR. Proton leak refers to the difference between OCR after oligomycin injection and non-mitochondrial OCR. Maximal respiration represents the difference between OCR after FCCP injection and non-mitochondrial OCR. Coupling efficiency is calculated as the percentage of ATP production rate to basal respiration rate. This method paper provides a detailed protocol to measure ECAR and OCR in lineage-negative HSPCs using the Seahorse XFe96 extracellular flux analyzer. This protocol describes approaches to isolate mouse lineage-negative HSPCs, explains the optimization of cell-seeding density and concentrations of various drugs used in extracellular flux assays, and describes drug treatment strategies.

Protocol

All vertebrate animal experiments were approved by and performed in accordance with the regulations of the University of Michigan Committee on Use and Care of Animals.

1. Day before the assay (Total time: ~10 min)

1. Hydration of the sensor cartridge (Step time: ~10 min)
   1. Open the extracellular flux assay kit and remove the sensor cartridge and utility plate assembly. Save loading guide flats for use the next day.
   2. Manually separate the sensor cartridge (the top green part with lid) from the utility plate (lower 96-well microplate) and place it upside-down next to the utility plate.
   3. Using a multichannel pipette, fill each well of the utility plate with 200 µL of calibrant, included with flux assay kit.
   4. Place the sensor cartridge back onto the utility plate, making sure to completely submerge the sensors in the calibrant.
   5. Place the assembled sensor cartridge and utility plate with calibrant in a non-CO₂ 37 °C incubator overnight. To prevent evaporation of the calibrant, ensure that the incubator is properly humidified. If using a regular oven incubator for non-CO₂ 37 °C incubations, place an open beaker containing water inside the incubator to humidify it. If available, use an XF prep station for all non-CO₂ 37 °C incubations.
      ​NOTE: Alternatively, the sensor cartridge can be hydrated overnight with 200 µL per well of sterile ultrapure water in a non-CO₂ 37 °C incubator. Replace water with 200 µL per well of 37 °C prewarmed calibrant, at least 45-60 min before loading the injection ports on the day of assay.

2. Day of the assay (Total time: ~9 h 30 min)

NOTE: The total time indicated above includes cumulative durations of steps 2.1-2.4 in addition to either step 2.5 or step 2.6.

1. Preparation of cell-adhesive-coated microplates (Step time: ~1 h 30 min)
   NOTE: Perform all steps in a biosafety cabinet.
   1. Prepare 2.5 mL of the cell adhesive solution (22.4 µg/mL, see the Table of Materials) per 96-well cell culture microplate by dissolving 56 µg of the cell adhesive in an appropriate volume of filter-sterilized 0.1 M sodium bicarbonate (pH 8.0) and immediately adding 1 N sodium hydroxide at half the volume of cell adhesive stock used. Vortex or pipette up and down to mix.
   2. Open the 96-well cell culture microplate (included with the flux assay kit) and dispense 25 µL of the prepared cell adhesive solution at the bottom of each well. Cover the microplate with the lid and incubate for 30 min at room temperature inside the hood.
   3. After incubation, remove and discard excess cell adhesive solution using a multichannel pipette or aspirator, and wash each well twice with 200 µL of sterile ultrapure water. Air-dry the plate, with the lid removed, inside the hood for 30-45 min.
      NOTE: Cell-adhesive-coated cell culture microplates may be stored for up to one week at 4 °C. Precoated microplates stored at 4 °C must be allowed to warm to room temperature inside the hood before seeding cells.
2. Preparation of assay media (Step time: ~30 min)
   1. Preparation of glycolysis stress test assay medium
      1. Supplement 100 mL of base medium (see the Table of Materials) with 1 mL of 200 mM L-glutamine.
         ​NOTE: The final L-glutamine concentration in the assay medium is 2 mM.
      2. Warm the L-glutamine-supplemented medium to 37 °C in a water bath.
      3. Adjust the pH of the warm medium to 7.4 with 1 N NaOH.
      4. Filter-sterilize the medium with a 0.2 µm filter and keep it at 37 °C until ready to use.
   2. Preparation of mitochondrial stress test assay medium
      1. Supplement 100 mL of the base medium with 0.45 g of glucose, 1 mL of 200 mM L-glutamine, and 1 mL of 100 mM sodium pyruvate.
         NOTE: The final assay medium contains 25 mM glucose, 2 mM L-glutamine, and 1 mM sodium pyruvate.
      2. Warm glucose, L-glutamine, and the sodium pyruvate-supplemented medium to 37 °C in a water bath.
      3. Adjust the pH of the warm medium to 7.4 with 1 N NaOH.
      4. Filter-sterilize medium with a 0.2 µm filter and keep at 37 °C until ready to use.
3. Harvest mouse lineage-negative HSPCs (Step time: ~3 h)
   1. Prepare the assay buffer by supplementing Hank's balanced salt solution with 4% fetal bovine serum. Prepare 1x enrichment buffer by diluting the 5x stock with sterile distilled water. Keep both buffers on ice until use.
   2. Humanely euthanize mice using CO₂ followed by cervical dislocation and remove the hindlimbs with scissors. Carefully remove all tissues from the bones, and cut the ends from both sides of the femur and tibia using scissors. Flush out bone marrow cells from the femur and tibia using the assay buffer. Pass the flushed cells through a sterile 70 µm filter, centrifuge the filtrate at 200 × g for 5 min at 4 °C, and discard the supernatant.
   3. Lyse the red blood cells by resuspending the cell pellet in 500 µL of ACK buffer (150 mM NH₄Cl, 10 mM KHCO₃, 0.1 mM EDTA, pH 7.2). Following lysis for 1 min on ice, wash the samples by adding 1 mL of assay buffer and centrifuge at 200 × g for 5 min at 4 °C. Discard the supernatant.
   4. After washing, incubate the samples with a cocktail of biotinylated antibodies directed against CD2 (1:200 dilution), CD3 (1:200 dilution), CD5 (1:200 dilution), CD8 (1:200 dilution), Ter-119 (1:200 dilution), B220 (1:200 dilution), and Gr-1 (1:800 dilution) for 45 min on ice in a total volume of 500 µL of assay buffer.
   5. Wash the samples with 1 mL of assay buffer with centrifugation as above.
   6. Wash the samples with 1 mL of 1x enrichment buffer with centrifugation as above.
   7. Incubate the samples with 20 µL of streptavidin nanobeads and 100 µL of 1x enrichment buffer on ice for 15 min.
   8. Wash the samples with 1 mL of 1x enrichment buffer with centrifugation as above.
   9. Resuspend the samples in 2.5 mL of 1x enrichment buffer. Place them on a separation magnet for 5 min. Collect the supernatants separately in 15 mL conical tubes.
   10. Resuspend magnet-separated samples in an additional 2.5 mL of 1x enrichment buffer, and place them again on the separation magnet for 5 min. Collect and combine supernatants to the prior collections in 15 mL conical tubes from step 2.3.9.
       NOTE: The supernatants contain the lineage-negative cell fractions.
   11. Centrifuge the 15 mL conical tubes containing the negatively selected cells for 5 min at 200 × g at 4 °C.
   12. Resuspend the cell pellets in 1 mL of assay buffer and count the cell number using trypan blue manually or via an automated cell counter such as a Countess 3.
       NOTE: Following the above-described approach, ~6 × 10⁶ lineage-negative HSPCs should be readily purified from the hindlimbs of a single mouse. If reagents, such as assay buffer, 1x enrichment buffer, and lineage-specific antibody cocktail, are prepared on the day prior to the experiment, it takes approximately 2.5-3 h to enrich HSPCs from 4 mice. It would take an additional 10 min for each mouse beyond this number.
4. Seeding cells in cell-adhesive-coated microplates (Step time: ~1 h)
   1. Centrifuge cells from step 2.3.12 at 200 × g for 5 min at room temperature.
   2. Remove the supernatant and resuspend the cell pellet in the appropriate assay medium (glycolysis stress test medium or mitochondrial stress test medium). Centrifuge at 200 × g for 5 min at room temperature.
   3. Repeat step 2.4.2. Remove the supernatant and resuspend the cells in the appropriate warmed assay medium to the concentration of 2.5 × 10⁵ cells per 50 µL or 5 × 10⁶ per mL.
   4. Pipette 50 µL of the cell suspension along the side of each well of the room-temperature cell-adhesive-coated 96-well cell culture microplate. Pipette 50 µL of the assay medium into the corner background measurement wells. Use a multichannel pipette for cell plating to ensure consistency.
   5. Create a centrifuge balance plate by adding 50 µL of water per well of a non-coated 96-well cell culture microplate.
   6. Centrifuge the cells in the plate at 200 × g for 1 min at room temperature. Do not apply brake. Transfer the plate to a non-CO₂ 37 °C incubator for 25-30 min to ensure the cells have completely attached. Visually confirm under a microscope that the cells are stably adhered to the microplate surface.
      NOTE: As ~6 × 10⁶ lineage-negative HSPCs can be harvested from the hindlimbs of a single mouse, HSPCs isolated from 4 mice (~2.4 × 10⁷ cells) are needed to fill an entire 96-well plate if the aim is to screen multiple interventions ex vivo in parallel. However, if the aim is to investigate the impact of a genetic alteration or an intervention on the metabolic parameters of HSPCs in vivo, then HSPCs isolated from multiple pairs of control and test mice can be analyzed in multiple technical replicates in parallel using a single plate.
5. Performing glycolysis stress test using the extracellular flux analyzer (Step time: ~3 h 30 min)
   1. Loading sensor cartridge with injecting compounds
      1. Prepare 100 mM glucose, 20 µM oligomycin, and 500 mM 2-DG solutions in prewarmed glycolysis stress test assay medium (pH 7.4).
         NOTE: All injecting compound solutions are made at 10x concentration. The final well concentrations are 10 mM for glucose, 2 µM for oligomycin, and 50 mM for 2-DG (see Table 1).
      2. Remove the hydrated sensor cartridge from the non-CO₂ 37 °C incubator from step 1.1.5. Remove air bubbles from the calibrant in the utility plate by lifting the sensor cartridge out of the calibrant and replacing it on to the same utility plate with the calibrant.
      3. Place the A/D loading guide flat (included in the extracellular flux assay kit) on the top of the sensor cartridge, orienting it so that the letter 'A' is located on the upper left-hand corner to ensure that only ports A are available for loading. Using a multichannel pipette, dispense 20 µL of 100 mM glucose solution in ports A.
      4. Replace the A/D loading guide flat with the B/C loading guide flat, orienting so that the letter 'B' is located on the upper left-hand corner to ensure that only ports B are available for loading. Using a multichannel pipette, dispense 22 µL of 20 µM oligomycin solution in ports B.
      5. Re-orient the B/C loading guide flat to locate the letter 'C' on the upper left-hand corner for loading ports C. Using a multichannel pipette, dispense 25 µL of 500 mM 2-DG solution in ports C.
      6. Remove and discard the loading guide flats.
         NOTE: It is important that each port series of all 96 wells, including those of the background wells, be loaded completely with the same volume of the injecting compound.
   2. Template creation, calibration, and measurements
      1. Create or load the template for the glycolysis stress test on the controller. Enter details regarding injection strategies, treatment conditions, and cell types, and press generate groups. Go to the plate map and assign wells to each group to be analyzed. Assign the 4 corner wells for background measurements.
      2. In protocol, make sure calibration and equilibration are checked in the initialization step.
      3. For baseline measurement and measurements after each injection (glucose, oligomycin, and 2-DG), set the number of measurement cycles to 3 and Mix - Wait - Measure times to 3 min - 0 min - 3 min (see Table 2).
      4. Remove the lid from the compounds loaded and hydrated sensor cartridge, submerged in calibrant in the utility plate. Place it on the work tray of the extracellular flux analyzer and begin the run.
         NOTE: The first step is the calibration, which usually takes ~20 min.
      5. Take out the microplate containing the cells from the non-CO₂ 37 °C incubator from step 2.4.6 after 25-30 min of incubation is over. Without disturbing the cells, slowly add 130 µL of the prewarmed glycolysis stress test assay medium (pH 7.4) per well to make up the medium volume in each well to 180 µL and return the plate to the non-CO₂ 37 °C incubator for additional 15-20 min.
         NOTE: A total incubation time of 45-60 min after centrifugation is preferred.
      6. After the calibration is over, replace the utility plate with the assay microplate (without lid) containing the cells. Press Load cell plate to start the measurements, which will take ~1.5 h for completion of the assay.
      7. After the measurements are over, collect the assay microplate containing the cells and remove the assay medium without disturbing the cells. Wash once gently with 250 µL of 1x phosphate-buffered saline without dislodging the cells.
      8. Add 10 µL of RIPA lysis buffer (50 mM Tris-HCl, pH 7.4, 1% NP-40, 0.5 % Na deoxycholate, 0.1% sodium dodecylsulfate, 150 mM NaCl, 2 mM EDTA, 50 mM NaF), supplemented with 1x protease inhibitor cocktail, to each well and agitate the plate on a shaker for 10 min. Freeze the whole plate at -80 °C.
      9. Thaw the plate, and perform a protein measurement assay for data normalization following the manufacturer's instructions.
      10. Retrieve and analyze the data. Open the data file using Wave Desktop Software. Click on Normalize and paste the normalization values for each well. Click on apply to normalize the data. Click on Export and select glycolysis stress test report generator to export the analyzed data to a report generator. Alternatively, export the data to an external application.
          NOTE: Alternatively, the total nuclear DNA content in each well can be used to normalize the data. A fluorescent dye, such as CyQuant that binds to nucleic acid, can be used to assess the total nuclear DNA content per well.
6. Performing a mitochondrial stress test using the extracellular flux analyzer (Step time: ~3 h 30 min)
   1. Loading sensor cartridge with injecting compounds
      1. Prepare 20 µM oligomycin, 20 µM FCCP, and 5 µM rotenone + 5 µM antimycin A solutions in prewarmed mitochondrial stress test assay medium (pH 7.4).
         NOTE: All injecting compound solutions are made at 10x concentration. The final well concentrations are 2 µM for oligomycin, 2 µM for FCCP, and 0.5 µM each for rotenone and antimycin A (see Table 3).
      2. Remove the hydrated sensor cartridge from the 37 °C incubator from step 1.1.5 and remove air bubbles as described previously in step 2.5.1.2.
      3. By following steps 2.5.1.3 to 2.5.1.6, dispense 20 µL of 20 µM oligomycin in ports A, 22 µL of 20 µM FCCP in ports B, and 25 µL of a mixture of 5 µM rotenone and 5 µM antimycin A in ports C.
         NOTE: It is important that each port series of all 96 wells, including those of the background wells, be loaded completely with the same volume of injecting compound.
   2. Template creation, calibration, and measurements
      1. Create or load the template for the mitochondrial stress test on the controller. Enter details regarding injection strategies, treatment conditions, and cell types, and press generate groups. Go to the plate map and assign wells to each group to be analyzed. Assign the 4 corner wells for background measurements.
      2. In protocol, make sure calibration and equilibration are checked in the initialization step.
      3. For baseline measurement and measurements after each injection (oligomycin, FCCP, and rotenone + antimycin A), set the number of measurement cycles to 3 and Mix - Wait - Measure times to 3 min - 0 min - 3 min (see Table 4).
      4. Start the run to perform the calibration as in step 2.5.2.4.
      5. Add 130 µL of the prewarmed mitochondrial stress test assay medium (pH 7.4) per well as in step 2.5.2.5.
      6. Start the measurements; retrieve and analyze the data as in steps 2.5.2.6 to 2.5.2.10. Export the analyzed data to the mitochondrial stress test report generator or an external application.

Results

Using this protocol, the cell number and the concentrations of various OxPHOS-targeting drugs (used in the extracellular flux assays) were optimized to measure ECAR and OCR of HSPCs isolated from 24-week-old female C57BL/6 mice. First, the glycolysis stress test was performed to optimize cell number and oligomycin concentration. A varying number of HSPCs per well ranging from 5 × 10⁴ to 2.5 × 10⁵ were used in this assay. As shown in Figure 2A and

Discussion

This method paper describes an optimized protocol for the assessment of cellular bioenergetics (glycolysis and OxPHOS) in mouse HSPCs using the Seahorse extracellular flux analyzer. This device is a powerful tool that simultaneously measures the ECAR and OCR of live cells, which are metrics of glycolysis and mitochondrial respiration, respectively. Thus, it can be used to assess the cellular bioenergetics in real time. Further, the 96-well microplate-based platform offers high-throughput quantification with high sensitiv...

Materials

Name	Company	Catalog Number	Comments
0.2 μm filter	Corning	430626	Used to filter-sterilize the assay media
100 mM sodium pyruvate	Life Technologies	11360-070	Component of mitochondrial stress test assay medium
15 mL conical Falcon tubes	Corning	352096	Used during HSPCs harvest and to prepare assay drug solutions
200 mM L-glutamine	Life Technologies	25030-081	Component of glycolysis stress test and mitochondrial stress test assay media
2-Deoxy-D-glucose (2-DG)	Sigma-Aldrich	D8375	3rd drug injection during glycolysis stress test
5x Enrichment buffer (MojoSort)	Biolegend	480017	Used for washings during HSPCs harvest
Ammonium chloride (NH4Cl)	Fisher Scientific	A661-3	Component of ACK lysis buffer
Antimycin A	Sigma-Aldrich	A8674	3rd drug injection during mitochondrial stress test
Bio-Rad DC protein assay kit	Bio-Rad	500-0112	Used as per manufacturer's instructions
Carbonyl cyanide-4 (trifluoromethoxy) phenylhydrazone (FCCP)	Sigma-Aldrich	C2920	2nd drug injection during mitochondrial stress test
Cell-Tak	Corning	354240	Cell adhesive. Used for coating cell microplates
Countes 3 Automated Cell Counter	ThermoFisher Scientific		For cell counting
EDTA	Fisher Scientific	O2793-500	Component of ACK lysis buffer and RIPA lysis buffer
Falcon 70 μm filter	Fisher Scientific	08-771-2	Used as cells strainer during HSPCs harvest
Gibco Fetal bovine serum (FBS)	Fisher Scientific	26400044	Used to prepare assay buffer during HSPCs harvest
Gibco HBSS	Fisher Scientific	14175095	Used to prepare assay buffer during HSPCs harvest
Glucose	Sigma-Aldrich	G7528	Component of mitochondrial stress test assay medium and first injection of glycolysis stress test
Oligomycin	Sigma-Aldrich	O4876	2nd drug injection during glycolysis stress test and 1st drug injection during mitochondrial stress test
PBS	Life Technologies	10010-049	Used to wash cells after assay for protein quantification
Potassium bicarbonate (KHCO3)	Fisher Scientific	P235-500	Component of ACK lysis buffer
Protease Inhibitor Cocktail (PIC)	Roche	11836170001	Supplied as tablets. One tablet was dissolved in 10 mL of RIPA buffer to make 1x PIC.
Rat biotin antimouse-B220, Clone ID: RA3-6B2	Biolegend	103203	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-CD2, Clone ID: RM2-5	Biolegend	100103	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-CD3, Clone ID: 17A2	Biolegend	100243	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-CD5, Clone ID: 53-7.3	Biolegend	100603	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-CD8, Clone ID: 53-6.7	Biolegend	100703	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-Gr-1, Clone ID: RB6-8C5	Biolegend	108403	Used for lineage depletion during HSPCs harvest
Rat biotin antimouse-Ter-119, Clone ID: TER-119	Biolegend	116203	Used for lineage depletion during HSPCs harvest
Rotenone	Sigma-Aldrich	R8875	3rd drug injection during mitochondrial stress test
Seahorse XFe96 extracellular flux analyzer	Seahorse Biosciences now Agilent		For ECAR and OCR measurments in real time.
Sodium bicarbonate	Sigma-Aldrich	S5761	Used to make Cell-adhesive solution for microplate coating
Sodium chloride (NaCl)	Fisher	BP358	Component of RIPA lysis buffer
Sodium deoxycholate	Sigma-Aldrich	D6750	Component of RIPA lysis buffer
Sodium Fluoride (NaF)	Sigma-Aldrich	S7920	Component of RIPA lysis buffer
Sodium hydroxide (NaOH)	Sigma-Aldrich	S8045	Prepared 1 N solution. Used for pH normalization
Streptavidin Nanobeads (MojoSort)	Biolegend	480015	Used for lineage depletion during HSPCs harvest
Tris-HCl	Fisher	BP153	Component of RIPA lysis buffer
XF base medium	Agilent	102353-100	base medium used to prepare glycolysis stress test and mitochondrial stress test assay media
XF prep station	Seahorse Biosciences		Used for non-CO2 37 °C incubations
XFe96 extracellular FluxPak	Agilent	102416-100 or 102601-100	Includes assay cartridges with utility plates, loading guide flats for loading drugs onto the assay cartridge, XF calibrant solution, and XF cell culture microplate