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JoVE Journal Cancer Research

Cancer Research

Isolation and Functional Assessment of Human Breast Cancer Stem Cells from Cell and Tissue Samples

Published: October 2, 2020 doi: 10.3791/61775
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1,2, 1,2, 1, 1,2, 1,2,3,4
1London Regional Cancer Program, 2Department of Anatomy & Cell Biology, Western University, 3Department of Oncology, Western University, 4Lawson Health Research Institute

Summary

This experimental protocol describes the isolation of BCSCs from breast cancer cell and tissue samples as well as the in vitro and in vivo assays that can be used to assess BCSC phenotype and function.

Abstract

Breast cancer stem cells (BCSCs) are cancer cells with inherited or acquired stem cell-like characteristics. Despite their low frequency, they are major contributors to breast cancer initiation, relapse, metastasis and therapy resistance. It is imperative to understand the biology of breast cancer stem cells in order to identify novel therapeutic targets to treat breast cancer. Breast cancer stem cells are isolated and characterized based on expression of unique cell surface markers such as CD44, CD24 and enzymatic activity of aldehyde dehydrogenase (ALDH). These ALDHhighCD44+CD24- cells constitute the BCSC population and can be isolated by fluorescence-activated cell sorting (FACS) for downstream functional studies. Depending on the scientific question, different in vitro and in vivo methods can be used to assess the functional characteristics of BCSCs. Here, we provide a detailed experimental protocol for isolation of human BCSCs from both heterogenous populations of breast cancer cells as well as primary tumor tissue obtained from breast cancer patients. In addition, we highlight downstream in vitro and in vivo functional assays including colony forming assays, mammosphere assays, 3D culture models and tumor xenograft assays that can be used to assess BCSC function.

Introduction

Understanding the cellular and molecular mechanisms of human breast cancer stem cells (BCSCs) is crucial for addressing the challenges encountered in breast cancer treatment. The emergence of the BCSC concept dates back to the early 21st century, where a small population of CD44+CD24-/low breast cancer cells were found to be capable of generating heterogenous tumors in mice1,2. Subsequently, it was observed that human breast cancer cells with high enzymatic activity of aldehyde dehydrogenase (ALDHhigh) also displayed similar stem cell-like properties3. These BCSCs represent a small population of cells capable of self-renewal and differentiation, contributing to the heterogenous nature of bulk tumors1,2,3. Accumulating evidence suggest that alterations in evolutionarily conserved signaling pathways drive BCSC survival and maintenance4,5,6,7,8,9,10,11,12,13,14. In addition, the cell extrinsic microenvironment has been shown to play a pivotal role in dictating different BCSC functions15,16,17. These molecular pathways and the external factors regulating BCSC function contribute to breast cancer relapse, metastasis18 and development of resistance to therapies19,20,21, with the residual existence of BCSCs post-treatment posing a major challenge to the overall survival of breast cancer patients22,23. Pre-clinical evaluation of these factors is therefore very important for identifying BCSC-targeting therapies that could be beneficial for achieving better treatment outcomes and improved overall survival in breast cancer patients.

Several in vitro human breast cancer cell line models and in vivo human xenograft models have been used to characterize BCSCs24,25,26,27,28,29. The ability of cell lines to continuously repopulate after every successive passage makes these an ideal model system to perform omics-based and pharmacogenomic studies. However, cell lines often fail to recapitulate the heterogeneity observed in patient samples. Hence, it is important to complement cell line data with patient-derived samples. Isolation of BCSCs in their purest form is important for enabling detailed characterization of BCSCs. Achieving this purity depends on the selection of phenotypic markers that are specific to BCSCs. Currently, the ALDHhighCD44+CD24- cell phenotype is most commonly used to distinguish and isolate human BCSCs from bulk breast cancer cell populations using fluorescence activated cell sorting (FACS) for maximum purity1,3,26. Furthermore, the properties of isolated BCSCs such as self-renewal, proliferation, and differentiation can be evaluated using in vitro and in vivo techniques.

For example, in vitro colony forming assays can be used to assess the ability of a single cell to self-renew to form a colony of 50 cells or more in presence of different treatment conditions30. Mammosphere assays can also be used to assess the self-renewal potential of breast cancer cells under anchorage-independent conditions. This assay measures the ability of single cells to generate and grow as spheres (mixture of BCSCs and non-BCSCs) at each successive passage in serum-free non-adherent culture conditions31. Additionally, 3-Dimensional (3D) culture models can be used to assess BCSC function, including cell-cell and cell-matrix interactions that closely recapitulate the in vivo microenvironment and allow investigation of the activity of potential BCSC-targeted therapies32. Despite the diverse applications of in vitro models, it is difficult to model the complexity of in vivo conditions using only in vitro assays. This challenge can be overcome by use of mouse xenograft models to evaluate BCSC behavior in vivo. In particular, such models serve as an ideal system for assessing breast cancer metastasis33, investigating interactions with the microenvironment during disease progression34, in vivo imaging35, and for predicting patient-specific toxicity and efficacy of antitumor agents34.

This protocol provides a detailed description for the isolation of human ALDHhighCD44+CD24- BCSCs at maximum purity from bulk populations of heterogenous breast cancer cells. We also provide a detailed description of three in vitro techniques (colony forming assay, mammosphere assay, and 3D culture model) and an in vivo tumor xenograft assay that can be used to assess different functions of BCSCs. These methods would be appropriate for use by investigators interested in isolating and characterizing BCSCs from human breast cancer cell lines or primary-patient derived breast cancer cells and tumor tissue for the purposes of understanding BCSC biology and/or investigating novel BCSC-targeting therapies.

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Protocol

Collection of patient-derived surgical or biopsy samples directly from consenting breast cancer patients were carried out under approved human ethics protocol approved by the institutional ethic board. All mice used to generate patient-derived xenograft models were maintained and housed in an institution approved animal facility. The tumor tissue from patient-derived xenograft models using mice were generated as per approved ethics protocol approved by the institutional animal care committee.

1. Preparation of cell lines

  1. Perform all cell culture and staining procedures under sterile conditions in a biosafety cabinet. Use sterile cell culture dishes/flasks and reagents.
  2. Maintain human breast cancer cells at 37 °C with 5% CO2 in defined media supplemented with fetal bovine serum (FBS) and necessary growth factors specific to each cell line.
  3. Maintain mouse NIH3T3 fibroblast cell cultures (for use in colony forming assays) at 37 °C with 5% CO2 in Dulbecco's Modified Eagle's Medium (DMEM) supplemented with 10% FBS.
  4. For all cultures, replenish the old media every 2-3 days with fresh media. Once the cultures reach 75-80% confluency, subculture into multiple sterile cell culture flasks.

2. Preparation of breast cancer tumor tissue

  1. Collect the patient-derived surgical or biopsy samples directly from consenting breast cancer patients under a human ethics protocol approved by the institutional ethics board.
  2. Subsequently, collect and generate tumor tissue from patient-derived xenograft models using mice under an animal ethics protocol approved by the institutional animal care committee.
  3. Collect all tumor tissues under sterile conditions into a 50 mL sterile conical tube containing 30 mL DMEM:F12 media, keep on ice, and process the samples as described below within 2 h of collection.

3. Generation of single cell suspensions of breast cancer cells

  1. Aspirate media from the flask containing a monolayer of breast cancer cells that is 60-80% confluent (cell lines of choice). Wash the cells with 1x phosphate buffered saline (PBS). Aspirate PBS and add appropriate cell dissociation solution (e.g., Trypsin:EDTA; just enough to cover the monolayer of cells) and incubate for 5 min at room temperature (recommended) or at 37 °C.
  2. Add 5 mL of culture media to neutralize the activity of cell dissociation solution.
  3. Transfer the resulting dissociated cell solution to a 50 mL conical tube and centrifuge at 1000 x g for 5 min.
  4. Discard supernatant and resuspended the cell pellet in 5 mL of 1x PBS. Count the cells using a hemocytometer and a microscope.
    NOTE: Observe for cell clumping in the hemocytometer. Repeat cell dissociation step if single cell suspension has not formed.
  5. After cell counting, re-centrifuge the cell suspension at 1000 x g for 5 min, discard supernatant, and resuspend the cell pellet in ALDH substrate buffer at a concentration of 1 x 106 cells/mL.

4. Generation of single cell suspension from tissue samples

  1. Mince the tumor tissue with surgical blades using a crisscross technique to obtain smaller pieces of approximately 1 mm in size. Transfer the tissue pieces into a fresh 50 mL conical tube containing 10 mL dissociation buffer (1X Collagenase in DMEM:F12). Seal the conical tube with parafilm and incubate at 37 °C in a shaker incubator for 40 min.
    NOTE: If there is not a shaker incubator, place the tube in a 37 °C water bath and mix the tube by vortexing every 5-10 min.
  2. Pellet the digested tissue by centrifuging sample at 530 x g for 5 min. Discard the supernatant and add 5 mL of trypsin. Pipette up and down using 1 mL pipette (set to 750 µL mark) to disrupt the pellet and incubate in a 37 °C water bath for 5 min. After incubation, pipette up and down vigorously to release single cells.
  3. Top up the total volume in the tube to 25 mL with DMEM:F12 media and centrifuge at 1000 x g for 5 min. Discard the supernatant and resuspend the pellet in 1 mL of dispase-DNase solution. Incubate in a 37 °C water bath for 5 min.
  4. Top up the total volume in the tube to 10 mL with PBS. Mix by pipetting up and down, pass the resulting cell suspension through a 40 µm cell strainer attached to a fresh 50 mL conical tube. Centrifuge at 1000 x g for 5 min.
  5. Discard supernatant and resuspend the cell pellet in 5 mL of 1x PBS. Count the cells and complete preparation of the cell suspension as described in steps 3.4 and 3.5.

5. Isolation of breast cancer stem cells (BCSCs)

  1. Label flow tubes for the unstained control, single cell staining controls (DEAB control, ALDH, CD44-PE, CD24-PE-Cy7, 7AAD), the negative control tube (stained with DEAB, CD44-PE, CD24-PE-Cy7 and 7AAD), fluorescent minus one (FMO) control and the ‘sort’ tube (stained with ALDH, CD44, CD24 and 7AAD).
  2. Transfer 500 μL (0.5 x 106 cells) of the cell suspensions from step 3.5 or step 4.5 to each tube that is labelled cells only, CD44, CD24 and 7AAD. Place the tubes on ice until use.
  3. Transfer 2 mL of sample (2 x 106 cells) to respective ‘ALDH’ tube. Add 5 μL of DEAB to the ‘DEAB control’ and ‘negative control’ tubes and cap it tightly. Add 10 μL of ALDH substrate to the ‘ALDH’ tube, mix well by vortexing, and immediately transfer 500 μL to corresponding ‘DEAB control’ and ‘negative control’ tube. Recap the ‘DEAB control’, ‘negative control’ and ‘ALDH tubes’ and incubate at 37 °C for 30-60 min (do not exceed 60 min).
    NOTE: The optimal incubation time may require optimization depending on the cell line. Always protect the ALDH substrate and the tubes containing stained cells from light.
  4. Following incubation, centrifuge all samples for 5 min at 250 x g. Resuspend the cells in 500 μL of ALDH substrate buffer. Add manufacturer-recommended or user-optimized concentration of anti-CD44-PE and anti-CD24-PE-Cy7 antibody cocktail and incubate at 4 °C for 30 min. Add anti-CD44-PE and anti-CD24-PE-Cy7 antibodies to respective ‘CD44’ and ‘CD24’ labelled tubes.
  5. Following incubation, centrifuge all samples at 250 x g for 5 min. Resuspend the cells in 500 μL of ALDH substrate buffer. Incubate the ‘negative control’ tube, ‘Sort tube’ and the ‘7ADD’ tube with 7AAD (suggested concentration: 0.25 µg/1 x 106 cells) for 10 min on ice.
    NOTE: The ALDH activity is detected in the green fluorescent channel, therefore a fluorochrome with a different compatible emission spectrum should be used. Where spectral overlap is observed during multi-parameter flow cytometry, single color controls and FMO control should be used as a guide to allow compensation between fluorochromes to minimize the spill over of fluorescent signal into other channels.
  6. Set up the analysis protocol on the FACS instrument in preparation for sample analysis. Create scatter plots (forward vs side scatter, forward scatter vs fluorescent channels).
  7. Using the unstained control, adjust the photomultiplier to separate debris from whole cell population and adjust the fluorescent voltage to move the whole cell population around the first log scale (101). Using the DEAB control, move the whole cell population within the second log scale (102) by adjusting the green fluorescent voltage channel.
  8. Analyze all the single staining controls first (ALDH, CD44-PE, CD24-PE-Cy7) and 7AAD and FMO control, adjusting the voltage to separate stained from unstained cells and to minimize the spillage of fluorescent signals into other channels.
  9. Gate on the positive population for each single stained cell sample. Using the negative control tube, gate for viability (7AAD negative), ALDHlow and ALDHhigh cell populations (representative gating strategy shown in Figure 1B).
  10. Analyze multiparameter stained samples of interest to isolate BCSCs. Using the viable ALDHlow and ALDHhigh gates, select for CD44+CD24- (BCSC) and CD44-CD24+ (non-BCSC) cell population respectively (Figure 1B).
  11. Collect viable BCSCs and non-BCSCs in collection media in sterile collection tubes (populations from two representative cell lines shown in Figure 2A&B). Use sorted cells for downstream in vitro and in vivo assays as described below.
    NOTE: In addition to in vitro and in vivo assays described below, BCSCs can be validated by measuring the expression of pluripotent markers such as SOX2, OCT4 and NANOG via standard immunoblotting techniques.

Figure 1
Figure 1: FACS gating strategy for isolation of BCSCs from breast cancer cell lines and tissue samples. (A) Flowchart describing the procedure of BCSC isolation. (B) Representative FACS plots showing the sort strategy used to isolate viable BCSCs and non-BCSCs from a heterogenous pool of cells. MDA-MB-231 human breast cancer cells are concurrently labeled with 7-AAD, CD44-APC, CD24-PE and the ALDH substrate. Cell subsets were isolated using a four-color protocol on a FACS machine. Cells are selected based on expected light scatter, then for singlets, and viability based on 7-AAD exclusion. Cells are then analyzed for ALDH activity and the top 20% most positive are selected as the ALDHhigh population, while the bottom 20% of cells with the lowest ALDH activity were deemed to be ALDHlow. Finally, 50% of the ALDHlow cells are further selected based on a CD44low/-CD24+ phenotype, and 50% of the ALDHhigh cells are selected based on CD44+CD24- phenotype. This figure has been adapted from Chu et al.17. Please click here to view a larger version of this figure.

Figure 2
Figure 2: BCSCs proportions are variable in different breast cancer cell lines. Representative image showing the differential proportion of BCSCs and non-BCSCs in (A) SUM159 and (B) MDA-MD-468 triple negative breast cancer cell lines following labelling and sorting as described in Figure 1. Please click here to view a larger version of this figure.

6. Colony forming assay

  1. Resuspend the cells of interest (sorted cells from step 5.11 or unsorted cells from steps 3.5 or 4.5) in complete media.
  2. Label three flow tubes for 1 x 102, 2 x 102 and 5 x 102 cells. Add 2 mL of complete media and transfer the appropriate cell number (sorted from step 5.11 or unsorted cells from steps 3.5 or 4.5) in respective tubes. Mix the cell solutions thoroughly by pipetting it up and down 5 times.
  3. Plate the cells in a 6-well plate and distribute the cell suspension by gently swirling the plates to obtain uniform distribution of cells.
  4. Incubate the plates in a 37 °C, 5% CO2 incubator until colonies appear (where colonies = ≥50 cells per colony). Carefully replenish media twice a week without disturbing colony formation.
  5. Aspirate media and wash once with 1 mL PBS. Add 0.5 mL of 0.05% crystal violet solution into each well and incubate the plate for 30 minutes. Remove excess crystal violet stain by washing with 2 mL of water. Repeat the washing step until background staining has been removed.
  6. Using a microscope at 4x and 10x magnification, count and record the total number of colonies generated (representative images shown in Figure 3A).
  7. Calculate the frequency of colony formation as follows: Frequency (%) = (# of colonies formed/number of cells seeded) x 100. For example, if 25 colonies are generated from 1 x 102 cells, then the Frequency of colony formation is, Frequency = (25/100) x100 = 25%.
  8. Alternatively, replace steps 6.1 to 6.4 with an alternate method involving co-culture with fibroblasts, which provide a microenvironmental support for BCSCs through production of necessary growth and survival factors.
  9. Pre-coat cell 60 mm culture dishes with type I bovine collagen (1 in 30 dilution of 3 mg/mL collagen). Allow collagen to polymerize for 30 min in a 37 °C incubator. Aspirate the unpolymerized collagen and wash the plate twice with 1x PBS. Cover the collagen-coated plate with 1 mL of PBS and set it aside at room temperature until use.
  10. Label three flow tubes for 1 x 103, 5 x 103 and 1 x 104 cells. Add 4 mL of colony forming assay media and transfer the appropriate number of cells (sorted from step 5.11 or unsorted cells from steps 3.5 or 4.5) into the respective tubes. Add irradiated mouse NIH3T3 fibroblasts (4 x 104 cells/mL of media). Mix cell solutions thoroughly by pipetting it up and down 5 times.
  11. Aspirate the PBS from the collagen-coated culture dish from step 6.1 and plate the cell mixture onto each of the cell culture plates as described in step 6.3.
  12. Incubate the plates in a 37 °C, 5% CO2 incubator and leave them undisturbed for 7-10 days or until colonies form, without replenishing the media. Count and record the total number of colonies generated as described in steps 6.6 and 6.7.

7. Mammosphere assay

  1. Resuspend the cells of interest (sorted cells from step 5.11 or unsorted cells from steps 3.5 or 4.5) in complete mammosphere media and plate cells at a seeding density of 5 x 102 cells/cm2 area in a 96 well ultra-low attachment cell culture plate.
    NOTE: Cell seeding density should be optimized for different cell lines.
  2. Incubate the culture plates for 5-10 days in a 37 °C incubator with 5% CO2. Carefully replenish media twice a week without disturbing mammosphere formation.
  3. After incubation, count the number of mammospheres generated in each well using a microscope; where mammospheres are defined as breast cancer cell clusters greater than 100 μm in diameter (representative images shown in Figure 3B).
  4. Calculate the mammosphere formation efficiency (MFE) as follows: MFE (%) = (number of mammospheres per well)/ (number of cells seeded per well) x 100 (i.e., if 5 mammospheres are generated by 1 x 102 cells in a well, then MFE = (5/100) x 100 = 5%).
  5. To subculture mammospheres, carefully transfer the media containing mammospheres content into a fresh 50 mL conical tube and centrifuge media at 1000 x g for 5 min. Carefully remove the supernatant, resuspend the cell pellet in 500 μL of trypsin, and incubate for 5 min at room temperature.
  6. Discard the supernatant and resuspend the pellet in 1 mL of complete mammosphere media. Count the cells using a hemocytometer and re-plate the cells in an ultra-low attachment cell culture plate as described in step 7.1.
    NOTE: In addition to sub-culturing, the mammosphere-derived cells can be also analyzed further by FACS to assess BCSC phenotype and/or obtain pure populations of BCSCs for other downstream assays.
  7. To determine the number of mammosphere-initiating cells contained within your cell populations, use an alternate method involving sphere limiting dilution analysis (SLDA). Plate cells in serial dilutions of high to low cell numbers in a 96 well ultra-low attachment cell culture plate, with the highest dilution resulting in less than one cell per well.
  8. Incubate the culture plate for 10-14 days in a 37 °C incubator with 5% CO2 and leave them undisturbed to avoid cell aggregation.
  9. After incubation, count the number of mammospheres generated in each well using a microscope; where mammospheres are defined as breast cancer cell clusters greater than 100 μm in diameter. Calculate the sphere-initiating frequency and significance using Extreme Limiting Dilution Analysis (ELDA) online software (http://bioinf.wehi.edu.au/software/elda/).

8. 3D culture model

  1. Depending on the experimental question, use basement membrane extract (BME) with or without growth factors (reduced). In order to evaluate the effect of individual growth factor on cancer cells, use growth factor reduced BME. It also helps in minimizing the non-specific effects of endogenous growth factors present in BME.
    NOTE: BME solidifies above 10 °C. Always keep BME on ice even during the thawing step.
  2. Carefully add 50 μL of BME per well in a 96-well plate without creating air bubbles and allow it to polymerize at 37 °C for 1 h. After 10 min of incubation, add 100 μL PBS to avoid drying of the gel layer.
  3. Resuspend the sorted cells from step 5.11 or unsorted cells from steps 3.5 or 4.5 at a concentration of 5 x 103 to 5 x 104/200 μL in 3D culture media.
  4. Once the BME has polymerized, remove PBS, add 200 µL of cell suspension to each well and incubate in 37 °C incubator with 5% CO2. Add PBS to the surrounding wells to avoid evaporation of the media.
    NOTE: The optimal number of cells for plating should be determined prior to setting of the experiment. Depending on the experimental question, BCSCs can be cultured alone or with other cells types (fibroblasts/endothelial/immune cells etc.).
  5. Add fresh media to the culture plates twice weekly. Maintain cultures for 10-14 days prior to analyzing the formation of organoids (representative images shown in Figure 3C).
  6. For sub-culturing, carefully aspirate the media and add 200 μL of dispase to each well containing cells. Incubate the plate in a 37 °C incubator for 1 h. Halfway through the incubation period (30 min), take out the plate, gently pipette the dispase solution up and down 5 times, and place back in the incubator for a further 30 min.
  7. After 1 h, transfer the dissociated cell solution to a flow tube. Wash the well with 1x PBS containing 2% FBS (fPBS) and transfer it to the flow tube. Centrifuge the tube at 1000 x g for 5 min. Carefully aspirate the supernatant and add 500 μL of trypsin, incubate at 37 °C for 5 min. Inactivate trypsin by adding equal amount of fPBS and centrifuge at 1000 x g for 5 min.
  8. Discard the supernatant and resuspend the pellet in 1 mL of 3D culture media. Count the cells and re-plate required number of cells in the BME as in steps 8.2 to 8.4.
    NOTE: Multiple wells can be pooled to further analyze or sort the cell population of interest.

Figure 3
Figure 3: In vitro assays to assess BCSC cell function. In vitro assays were performed as described in protocol sections 6.1 to 6.5 (A), 7.1 to 7.4 (B), or 81. to 8.4 + 8.6 (C). (A) Representative image showing the colonies generated by MDA-MB-231 human breast cancer cells; (B) Representative images showing mammosphere formation by MCF7, SUM159, or MDA-MB-468 human cell lines as well as patient-derived LRCP17 breast cancer cells. (C) Representative images showing the 3D structures formed by MCF7 and MDA-MB-231 breast cancer cells in 3D cultures models. Please click here to view a larger version of this figure.

NOTE: Perform animal experiments under an animal ethics protocol approved by the institutional animal care committee.

9. In vivo xenograft model

  1. In order to determine the tumor initiation capacity of breast cancer stem cells, prepare cells (sorted population from step 5.7 or unsorted populations from steps 3.5 or 4.5) using a limiting dilution approach. Serially dilute cells in PBS using between 1 and 5 different dilution groups, with doses as low as 0.01-0.2 x 102 cells/100 µL and as high as 1 x 106 cells/100 µL.
    NOTE: Unsorted/whole population cells can be used as a control. The number of dilution groups used will depend on the desired scientific outcome (e.g. if only testing tumorgenicity then 1 group at a higher cell number may be used, whereas when calculating tumor-initiating capacity, it is optimal to test 5 limiting dilution doses).
  2. To generate xenograft models from human breast cancer cells, use immunocompromised female mice (athymic nude [nu/nu], nonobese diabetic/severe combined immunodeficient [NOD/SCID] or NOD/SCID IL2γ [NGS] strains).
    NOTE: Although a minimum of 4 animals per group can be used, 8-12 animals per group is recommended to obtain robust results particularly for limiting dilution analysis.
  3. Perform standard mammary fat pad (MFP) injections using 100 µL/mouse of each cell preparation, under sterile conditions in a biosafety cabinet.
    NOTE: For optimal breast tumor growth and spontaneous metastasis to distant organs, the thoracic MFP is recommended. Alternatively, the inguinal MFP can also be used.
  4. Post-injection, monitor the mice on a daily basis for general health and tumor growth at the site of injection. Upon detection of a palpable tumor, begin measuring the tumor size by calipers in two perpendicular dimensions and record weekly until endpoint.
    NOTE: The experimental end point is determined based on the regulations laid out the institutional animal ethics protocol; typically, endpoint by euthanasia is usually required once tumor volumes reach 1500 mm3. For BCSC populations and/or higher cell doses (e.g. >1 x 104 cells), this endpoint will likely be reached within 4-8 weeks of MFP injection. For very low cell doses and/or non-BCSC cell populations, tumor growth should be allowed to progress for up to 8 months post-injection.
  5. From these measurements, calculate the tumor volume using the following formula: Volume in mm3 = 0.52 x (width)2 x length. If using a limiting dilution approach, calculate tumor-initiating capacity and significance using ELDA online software (http://bioinf.wehi.edu.au/software/elda/).
  6. Alternatively, to humanely extend the endpoint, surgically remove primary tumors and continue to monitor mice for health and/or development of spontaneous metastasis in distant organs. Use resected tumor tissue for the generation of serial xenotransplants.
  7. At endpoint, harvest tissue from primary tumors and distant organs (lymph nodes, lung, liver, brain, bone) and carry out histopathological and/or immunohistochemical analysis or dissociated the tumor tissue and use in the in vitro assays described in sections 6-8.

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Representative Results

The described protocol allows isolation of human BCSCs from a heterogenous population of breast cancer cells, either from cell lines or from dissociated tumor tissue. For any given cell line or tissue sample, it is crucial to generate a uniform single cell suspension to isolate BCSCs at maximum purity as contaminating non-BCSC populations could result in variable cellular responses, especially if the study aim is to evaluate the efficacy of therapeutic agents targeting BCSCs. Application of a stringent sorting strategy will minimize the presence of contaminating non-BCSCs and result in the ability to collect the proportion of breast cancer cells with stem cell-like characteristics that display a cellular phenotype that distinguishes them from bulk population of cancer cells. Human breast cancer cells that exhibit enhanced ALDH enzymatic activity, express high levels of the cell surface marker CD44, and low/negative expression of CD24 have an ALDHhighCD44+CD24- phenotype and can be classified as BCSCs. The proportion of BCSCs within the bulk population can vary between cell lines or patients (Figure 2), and often depends on disease stage, with more aggressive breast cancer usually displaying a higher proportion of BCSCs26,36,37.

Isolated BCSCs can be used to perform different in vitro and in vivo assays where their behavior and function can be compared to that of the bulk and/or non-BCSC populations. For example, the ability of a single breast cancer cell to self-renew and generate colonies of 50 cells can be assessed by colony-forming assays (Figure 3A). The ability of BCSCs to self-renew under anchorage-independent experimental conditions can be assessed by mammosphere assays, where variable sphere number, size, and sphere-initiating capacity can be analyzed and correlated with the presence and function of BCSCs (Figure 3B). It is important to determine the seeding cell densities for different breast cancer cell lines or breast tumor samples to obtain optimal results. This is particularly important when performing SLDA, as higher cell densities could lead to cell aggregation resulting in misinterpretation of cellular activity.

Culturing breast cancer cells in BME allows BCSCs to form 3D structures that recapitulate in vivo conditions (Figure 3C). 3D culture of breast cancer cells in the presence of other microenvironmental cell types such as fibroblasts, endothelial cells, and/or immune cells has the added capacity for investigating the role of microenvironment in 3D growth of BCSCs38,39. The specific cell numbers required to generate 3D organoids may vary depending on the cell line or patient tumor source, and thus it is important to optimize the culture conditions and cell numbers prior to any large-scale experiments.

Finally, in vivo mouse xenograft models can be used to understand the differences in growth (Figure 4) self-renewal, differentiation and/or tumor-initiating ability of BCSCs in vivo compared to non-BCSCs or bulk cell populations. Often, the in vitro cellular responses observed in the presence of exogenous factors or therapeutic agents is not representative of in vivo setting, suggesting that in vitro observation should be complimented with in vivo studies whenever feasible. Using in vivo xenograft models, the cellular heterogeneity and tumor architecture is preserved and thus these models can serve as a system that closely mimics the microenvironment in human patients. In vivo LDA can be performed to determine the proportion of tumor-initiating cells in a given mixed population of cancer cells (BCSCs or non-BCSCs)40,41. The range of cell dilutions used should be optimized and will depend on the frequency of initiating cells in the cell population of interest. Ideally these dilutions should include doses that result in 100% tumor formation, down to cell doses with no tumor formation and a reasonable range in between. The frequency of tumor-initiating cells in primary samples can be variable, and in instances where breast tumors have very low numbers or heterogenous populations of tumor-initiating cells, performing LDA can be particularly challenging42. In these cases, injecting larger number of cells would be more appropriate for understanding breast cancer biology.

Figure 4
Figure 4: In vivo xenograft assays to assess BCSC function. MDA-MB-231 breast cancer cells were isolated by FACS as described in Figure 1 and injected into the right thoracic mammary fat pad of female NSG mice as described in protocol sections 9.1 to 9.8 (5 x 105 cells/mouse; 4 mice/cell population). Primary breast tumor growth kinetics are shown for ALDHhiCD44+CD24- (■) versus ALDHlowCD44low/-CD24+ (□) populations. Data represented as the mean ± S.E.M. * = significantly different tumor size than respective ALDHlowCD44low/- subsets at the same time-point (P < 0.05). This figure has been adapted from Croker et al.26. Please click here to view a larger version of this figure.

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Discussion

Breast cancer metastasis and resistance to therapy have become major cause of mortality in women worldwide. The existence of a sub-population of breast cancer stem cells (BCSCs) contributes to enhanced metastasis26,43,44,45,46 and therapy resistance21,47,48. Therefore, the focus of future treatments should aim at eradicating BCSCs to achieve better treatment outcomes, and this requires accurate methods for isolating and characterizing the functional characteristics of BCSCs using both in vitro and in vivo methods.

Immortalized cell lines derived from different subtypes of breast cancer have proven to be feasible models to study breast cancer biology including the isolation and characterization of BCSCs26,49,50. The high proliferative capacity and unlimited expansion ability of cell lines provides an ideal model system for performing studies that are highly reproducible and technically straightforward. However, due to the clonal origin of cell lines, they may fail to recapitulate the heterogeneity exhibited by different patients and/or by cancer cells within tumor tissue. In addition, genetic alterations can be acquired during serial passaging of cell lines and may induce genotypic or phenotypic changes that can confound experimental results51. In contrast, primary patient-derived cells, despite their limited proliferative and expansion ability, may provide a more accurate model to that observed in vivo. However, such samples may be more difficult to acquire and be more technically challenging to work with. All of these factors should be considered when choosing a starting model system with which to isolate and characterize BCSCs.

FACS is a commonly used technique to isolate cells of interest based on cell surface marker expression52,53. Based on cell surface antigens (CD44 and CD24) and ALDH enzymatic activity, human BCSCs can be isolated at high purity from both breast cancer cell lines and tumor tissues1,2. The sorting efficiency determines the purity of sorted sample, and it is recommended that users analyze a small portion of sorted sample incubated with viability dye to check the efficiency of sorting53,54. The sorting efficiency can be confounded by many factors including the presence of cell clumps, a high number of dead or dying cells, improper compensation of the fluorochromes and/or damage to cell surface antigens due to sensitivity to trypsin or collagenase during pre-sorting dissociation steps53,54,55,56. Therefore, generation of a proper single cell suspension and use of appropriate cell dissociation techniques will increase the sorting efficiency. While performing multiparameter cell sorting, it is important to choose fluorochromes that minimizes spectral overlap. In some cases, where spectral overlap cannot be avoided, a control that contains all the fluorochromes except one (fluorescence minus one, FMO) should be used to minimize the spillover of fluorescent signals into other channels54. Alternatively, the spectral overlap can reduced by immunomagnetically isolating cell populations prior to final FACS isolation of cells of interest56.

In vitro assays such as the colony-forming and mammosphere assays described in this protocol have been extensively used to study the self-renewal and proliferative ability of BCSCs57,58,59,60,61,62. Additionally, these assays can be used to assess the activity of different therapeutic drugs on BCSC function. Several evolutionarily conserved signaling pathways have been implemented in BCSC maintenance63, and both colony-forming64,65,66 and mammosphere assays64,67 have been used to assess the value of therapeutic disruption of these pathways as an intervention to block BCSC intrinsic signaling and reduce BCSC activity and disease progression. Colony forming assay using primary cells can be challenging due to low cell density, variation between samples and lack of its adaptability to isolated in vitro conditions. These challenges can be overcome by culturing BCSCs on a soft agar layer or by coculturing them with fibroblasts on a collagen-coated cell culture dish68,69,70. In addition, supplementing growth factors into the culture media (such as FGF771) could also improve the colony-forming ability of cells isolated from tissue samples. In addition, over-digestion of tissue using collagenase or trypsin during single cell suspension generation step can result in low to zero colony-forming ability and reduce mammosphere-forming efficiency31. In both assays, care should be taken to incubate the assay plates undisturbed to avoid disruption of colony or sphere structures as they are forming. It is also recommended that users extend the incubation period for primary cells (relative to cell lines) as it might take longer for these cells to form colonies or spheres.

Multiple lines of evidence have demonstrated the critical role of extracellular matrix (ECM)15,17,72 and stromal components, such as fibroblasts, immune cells, endothelial cells and adipocytes in influencing BCSC functions15. Thus, the 3D culture model we describe in this protocol can provide a useful experimental system for helping to recapitulate the in vivo tumor microenvironment in an in vitro setting. Although the 3D culture system closely resembles the tumor microenvironment in cancer patients, long term maintenance of cells as organoids can be difficult. In addition, optimization of the 3D culture conditions and the ability to accurately investigate self-renewal and differentiation ability of BCSCs is challenging73. The efficiency of organoids formed in 3D culture system depends on the growth factors supplemented in the culture media74. Absence of key components (for example, ROCK inhibitor) could lead to reduced or no organoid formation74. Media should be replenished every 3-4 days to maintain optimal cellular function and the sustainability of the culture. In order to recapitulate in vivo conditions and response, it is always important to allow the cells to form organoids prior to any kind of exogenous treatment75. Cells derived from patient samples should be giving sufficient time to form organoids, particularly if the objective is the evaluate drug response75.

While these in vitro methods are attractive and accessible experimental tools for characterizing BCSC function, tumor heterogeneity and the effect of tumor microenvironment on BCSC behavior cannot be studied with complete effectiveness. These in vitro assays should therefore be complemented with in vivo xenograft models whenever feasible in order to further validate experimental findings related to BSCS biology and/or response to novel therapeutics. Different in vivo models have been used study BCSC tumorigenicity and metastasis. Ectopic (subcutaneous engraftment) and orthotopic (MFP engraftment) mouse models have been used to generate breast tumors and assess longitudinal changes in tumor growth over time50. Although both in vivo injection approaches can be used to study BCSC biology, the native stromal and vasculature-related components of the MFP allow more accurate recapitulation of primary breast tumor progression as observed in patients, and thus MFP injection is preferred76,77,78. Finally, the use of immunocompromised mice is required for engraftment of human BCSCs and tumor growth, and this prevents incorporating the role of immune cells in tumorigenesis and metastasis studies79. More recently, this limitation has been addressed through the use of humanized mice in which a human immune system is reconstituted via bone marrow transplantation prior to the initiation of xenograft studies80,81,82. However, these models are expensive and technically challenging, and thus are still not commonly used83.

In summary, here we have provided a protocol for the isolation of human BCSCs from both breast cancer cell lines and patient-derived tumor tissue samples. We have also described in vitro and in vivo protocols for downstream assays that can be used to study BCSC function, with the ability to be optimized for different breast cancer cell sources and the flexibility to be performed under different experimental conditions. These protocols will be useful for investigators interested in cancer stem cells, breast cancer biology and therapeutic development, with the ultimate goal of improving patient outcomes in the future.

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Disclosures

The authors have nothing to disclose.

Acknowledgments

We thank members of our laboratory for their helpful discussions and support. Our research on breast cancer stem cells and the tumor microenvironment is funded by grants from the Canadian Cancer Research Society Research Institute and the U.S. Army Department of Defense Breast Cancer Program (Grant # BC160912). V.B. is supported by a Western Postdoctoral Fellowship (Western University), and both A.L.A. and V.B. are supported by the Breast Cancer Society of Canada. C.L. is supported by a Vanier Canada Graduate Scholarship from the Government of Canada.

Materials

Name Company Catalog Number Comments
7-Aminoactinomycin D (7AAD) BD 51-68981E suggested: 0.25 µg/1x106 cells
Acetone Fisher A18-1
Aldehyde dehydrogenase (ALDH) substrate Stemcell Technologies 1700 Sold commerically as part of the ALDEFLOUR Assay kit; follow manufacturer's instructions for ALDH substrate preparation
Basement membrane extract (BME) Corning 354234 Sold under the commercial name Matrigel
Cell culture plates: 6 well Corning 877218
Cell culture plates: 60mm Corning 353002
Cell culture plates: 96-well ultra low attachment Corning 3474
Cell strainer: 40 micron BD 352340
Collagen Stemcell Technologies 7001 Prepare 1:30 dilution of 3 mg/mL collagen in PBS
Collagenase Sigma 11088807001 1x
Conical tubes: 50 mL Fisher scientific 05-539-7
Crystal violet Sigma C6158 Use 0.05% crystal violet solution in water for staining
Dispase Stemcell Technologies 7913 5U/mL
DMEM:F12 Gibco 11330-032 1x, With L-glutamine and 15 mM HEPES
DNAse Sigma D5052 0.1 mg/mL final concentration
FBS Avantor Seradigm Lifescience 97068-085  
Flow tubes: 5ml BD 352063 Polypropylene round-bottom tubes
Methanol Fisher 84124
mouse anti-Human CD24 antibody BD 561646 R-phycoerythrin and Cyanine dye conjugated Clone: ML5
mouse anti-Human CD44 antibody BD 555479 R-phycoerythrin conjugated, Clone: G44-26
N,N-diethylaminobenzaldehyde (DEAB) Stemcell Technologies 1700 Sold commerically as part of the ALDEFLOUR Assay kit; follow manufacturer's instructions DEAB preparation
PBS Wisent Inc 311-425-CL 1x, Without calcium and magnesium
Trypsin-EDTA Gibco 25200-056
Mammosphere Media Composition
B27 Gibco 17504-44 1x
bFGF Sigma F2006 10 ng/mL
BSA Bioshop ALB003 04%
DMEM:F12 Gibco 11330-032 1x, With L-glutamine and 15 mM HEPES
EGF Sigma E9644 20 ng/mL
Insulin Sigma 16634 5 µg/mL
3D Organoid Media Composition
A8301 Tocris 2939 500 nM
B27 Gibco 17504-44 1x
DMEM:F12 Gibco 11330-032 1x, With L-glutamine and 15 mM HEPES
EGF Sigma E9644 5 ng/mL
FGF10 Peprotech 100-26 20 ng/mL
FGF7 Peprotech 100-19 5 ng/mL
GlutaMax Invitrogen 35050-061 1x
HEPES Gibco 15630-080 10 mM
N-acetylcysteine Sigma A9165 1.25 mM
Neuregulin β1 Peprotech 100-03 5 nM
Nicotinamide Sigma N0636 5 mM
Noggin Peprotech 120-10C 100 ng/mL
R-spondin3 R&D 3500 250 ng/mL
SB202190 Sigma S7067 500 nM
Y-27632 Tocris 1254 5 µM

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Tags

Isolation Functional Assessment Breast Cancer Stem Cells Cell And Tissue Samples In Vitro In Vivo Characterization Assays Molecular Events Tumorigenicity Metastasis Therapeutic Strategies Single Cell Suspension Cell Dissociation Solution Culture Medium ALDH Substrate Buffer Tissue Sample Surgical Blades Dissociation Buffer
Isolation and Functional Assessment of Human Breast Cancer Stem Cells from Cell and Tissue Samples
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Bhat, V., Lefebvre, C., Goodale, D., … More

Bhat, V., Lefebvre, C., Goodale, D., Rodriguez-Torres, M., Allan, A. L. Isolation and Functional Assessment of Human Breast Cancer Stem Cells from Cell and Tissue Samples. J. Vis. Exp. (164), e61775, doi:10.3791/61775 (2020).

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