Targeting specificity of dendritic cells on breast cancer stem cells: in vitro and in vivo evaluations

Introduction

Breast cancer is the most common cancer in women both in developed and in developing countries. According to Global Health Estimates 2013 (WHO), breast cancer caused over 508,000 female deaths worldwide in 2011. In 2013, the average survival period of breast cancer was 5 years, however, this period is lower in developing countries with similar distributions of the stage at diagnosis.¹ For many years, the only standardized treatment options for cancer have been surgery, radiotherapy, and chemotherapy. However, many cases are complicated by tumor relapse and resistance to chemotherapy.² Therefore, it is necessary to develop new therapies that are less toxic and more effective. Because of the importance of cancer stem cells in tumors, many researchers are trying to isolate these cells to study their functional properties and evaluate whether they can effectively treat cancer. Recently, there have been many reports showing the prospective isolation of cancer stem cells in numerous malignancies, including breast,³ brain,⁴ colon,⁵ head and neck,⁶ pancreatic,⁷ melanoma,⁸ hepatic carcinoma,⁹ lung,¹⁰ prostate,¹¹ and ovarian tumors.¹² These cancer stem cells have therefore become targets for cancer treatment.

In recent years, dendritic cell (DC)-based therapy has shown promise as a cancer treatment. DCs were first discovered by Steinman and Cohn,¹³ and are professional antigen-presenting cells that have the ability to activate both innate and adaptive immune responses. DCs have the unique ability of cross-presentation, because they process and present peptide fragments on the surface of MHC class I and MHC class II molecules.¹⁴ After maturation, DCs migrate to the draining lymph node and activate naïve T cells. Immature DCs are more efficient than mature DCs at capturing and processing antigens. However, mature DCs are more efficient at activating and stimulating T cells.^15–18 These mature DCs are more efficient than immature DCs at homing to lymph nodes.^19,20 Immature DCs can be generated in vitro in the presence of cytokines GM-CSF and IL-4, and then mature when primed in vitro with tumor-specific antigens used for cancer treatment.^21,22

To date, some studies have used DC-specific antigens to treat breast tumors and reported that DC treatment is effective for reducing tumor mass.^23–25 These results have opened the door for DC therapy as a novel approach in breast cancer treatment. However, these studies targeted tumor or cancer cells. In order to improve the efficiency of this therapy, some recent studies developed DC therapy targeting cancer stem cells,²⁶ such as breast²⁷ and glioblastoma cancer stem cells.²⁸ More importantly, targeting glioblastoma cancer stem cells by DC therapy was permitted in a clinical trial (NCT00846456).

However, to the best of our knowledge, no study has addressed the specific effects of DCs on cancer stem cells or stem cells. This study evaluates the specificity of DC therapy primed with breast cancer stem cells (BCSCs) in breast cancer treatment. We investigated the specific inhibition of DCs and induced cytotoxic T lymphocytes (CTLs) in vitro and in vivo.

Materials and methods

4T1 culture

Murine 4T1 mammary gland tumor cells, which are spontaneously metastatic tumor cells derived from BABL/c mice, were purchased from the American Type Culture Collection (ATCC). Murine 4T1 mammary gland tumor cells are comparable to human stage IV breast cancer. The tumor cells were cultured in RPMI 1640 medium (Sigma-Aldrich, St Louis, MO, USA) and supplemented with 10% fetal bovine serum (FBS; Sigma-Aldrich) as well as 1× antibiotic mycotic (Sigma-Aldrich) in 25 mL cell culture flasks. The culture medium was regularly changed at 3-day intervals.

Verapamil cytotoxicity assay

The 4T1 cells were cultured in culture medium supplemented with various levels of verapamil from 0 to 100 μg/mL. The cytotoxicity effect of verapamil on 4T1 cells was measured by the xCELLigence Real-Time Cell Analyzer (RTCA) (Hoffmann-La Roche Ltd., Basel, Switzerland). This system monitored cellular events such as cell number, adhesion, viability, and morphology in real time by measuring the change in electrical impedance as the living cells interacted with the biocompatible microelectrode surface in the E-plate well. The final cell density was 5 cells per well in 200 μL RPMI-10% FBS. After 24 hours of culture to allow cell adhesion and spreading, all of the RPMI-10% FBS was removed, transferred, and supplemented with 0, 10, 20, 30, 40, 50, 60, 70, 80, 90, and 100 μg/mL verapamil (Sigma-Aldrich). Each concentration of verapamil was repeated in three different wells. The highest concentration of verapamil in which 4T1 cells could survive was used to select verapamil-resistant 4T1 cells for further experiments.

Stemness of verapamil-resistant 4T1 cells

The stemness of verapamil-resistant 4T1 cells was evaluated by assays including mammosphere culture, ALDH expression, and in vivo tumorigenesis. The verapamil-treated and -untreated 4T1 cells were placed in culture flasks in serum-free DMEM-F12, supplemented with 10 ng/mL basic fibroblast growth factor, 20 ng/mL epidermal growth factor, 5 ng/mL insulin, and 0.4% bovine serum albumin at 37°C, 5% CO₂ in a humidified chamber. The culture flasks were placed vertically. Culture medium was changed at 3-day intervals. After 10 days of culture, the number and diameter of spheres were determined using an inverted microscope at 20× magnification. ALDH expression was evaluated using an ALDEFLUOR kit (Stemcell Technologies, Vancouver, British Columbia, Canada) according to the manufacturer’s instructions. Immune-deficient mice were used to test the tumorigenicity of BCSC candidates. Immunodeficient mice were administered busulfan intramuscularly through abdominal muscles, and cyclophosphamide intravenously via the tail vein at doses of 20 and 200 mg/kg, respectively.

Bone marrow-derived mesenchymal stem cell isolation and proliferation

Mesenchymal stem cells (MSCs) were isolated from murine bone marrow. Mononuclear cells were cultured in medium DMEM/F12 supplemented with 10% FBS and 1% antibiotic mycotic (Sigma-Aldrich). MSC candidates were subcultured for five passages, and the stemness of MSCs was checked according to Dominici’s guidelines.²⁹ Cells were evaluated by marker expression of CD44, CD73, CD90, CD105, CD14, CD34, and CD45 by flow cytometry; cells were then differentiated into adipocytes, osteoblasts, and chondrocytes.

Antigen generation

Both verapamil-resistant 4T1 cells and MSCs at a concentration of 5×10⁶ cells/mL were suspended in PBSA. Cells were rapidly frozen at −196°C and thawed at 37°C. This freeze–thaw process was repeated 3 times. Protein was harvested by PRO-PREP instructions (Intron Biotechnology, Seongnam-si, Gyeonggi-do, Korea). In brief, after centrifugation, the cell pellet was suspended in 1 mL cold PRO-PREP solution. The mix was centrifuged at 13,000 rpm at 4°C. The supernatant containing the expected protein was collected and stored at −80°C. Protein concentration was determined by Bradford assay.

Generation of DCs from mouse bone marrow-derived mononuclear cells

Mouse bone marrow cells were harvested by flushing the marrow cavities of the femur and tibia bones of male mice with medium under aseptic conditions. The harvested marrow was depleted of erythrocytes and cultured only in complete RPMI-10% FBS. On day 2, the cultured medium was changed with RPMI-10% FBS, 100 ng/mL granulocyte monocyte colony-stimulating factor (GM-CSF), and 50 ng/mL IL-4 (Santa Cruz Biotechnology Inc., Dallas, TX, USA). Half of the medium was replaced with fresh medium containing the same cocktail of cytokines every 2 days. On day 8, antigens were added into the cultured medium at a concentration of 500 ng/mL. On day 10, nonadherent fractions of DCs were harvested. Adherent fractions of DCs were also harvested by incubating with 0.25% Trypsin/EDTA (Sigma-Aldrich). Then, the numbers of harvested DCs were determined by automatic counting using a Nucleocounter^® (ChemoMetec A/S, Allerod, Denmark).

Mature DCs generated from mouse bone marrow were directly stained using fluorescent-conjugated monoclonal antibodies, including anti-CD40, CD80, CD83, and CD86, for 30 minutes at 4°C in the dark. Cells were then analyzed using FACSCalibur flow cytometry (BD Biosciences, San Jose, CA, USA) with CellQuest software.

In vitro evaluation of DC-based vaccination

To evaluate the effects of DCs on BCSCs, we developed a system using xCELLigence RTCA equipment. xCELLigence RTCA was used to evaluate cell proliferation and cytotoxicity on the basis of changes in electrical impedance on the surface of the E-plate, a plate with electric nodes on the surface allowing measurement of changes in impedance (Table 1).

Table 1 Experimental groups and their descriptions Abbreviations: BCSC, breast cancer stem cell; CTL, cytotoxic T lymphocyte; DC, dendritic cell; MSC, mesenchymal stem cell.

We observed differences in adherence of BCSCs, DCs, and CTLs. BCSCs were strongly attached to the surface of the E-plate, while DCs and lymphocytes were weakly attached. Thus, on the basis of BCSC proliferation on the E-plate with or without DCs or CTLs, we could determine the cytotoxic effects of this therapy on target cells. From 0 to 24 hours, verapamil-resistant cells (VRCs) were cultured as adherent cells in the E-plate (96 wells) in groups 1 and 3–6, while group 2 had DCs and CTLs added. After 24 hours, cells in groups 1–6 had fresh medium added. Only fresh culture medium was added to groups 1 and 2, while DC-induced CTLs were added to groups 3–6. Before this, mature DCs (BCSC-DCs and MSC-DCs) were incubated with CTLs at different ratios of DCs and CTLs, ie, 1:10 and 1:40, over the course of 24 hours. These mixtures of DCs and CTLs were added to the E-plate wells containing BCSCs. Finally, the E-plates were then placed on the xCELLigence instrument to monitor BCSC proliferation. CTLs were prepared according to a previously published study.³⁰

Breast tumor-bearing mouse models and in vivo assay

The male mice were housed in an animal maintenance facility. The soda bedding was changed at 4-day intervals. All experiments on animals were performed in accordance with the guidelines approved by the Ethics Committee of Stem Cell Research and Application Laboratory, University of Science, VNU-HCM. Fifty μL of verapamil-resistant 4T1 cells (10⁶ cells) were injected into the mammary pads of 8-week-old mice.

Tumors formed after 2 days. The animals with tumors were divided into 4 groups of 4 mice each. The control group (group 1) was intravenously injected with RPMI 1640. The second group (group 2) was intravenously injected with DCs primed with mouse MSC-derived antigen (MSC-DC). Group 3 was treated with DCs primed with verapamil-resistant 4T1-derived antigen (BCSC-DC) by injection into the tumor. The tumor lengths were measured daily. Survival, symptoms of pain, and inflammation were monitored. Any mice expressing abnormal symptoms were isolated from the groups and closely observed. After the last experiment, all mice were euthanized to collect and measure the tumors.

CD4 and CD8 analysis

Two days after treatment, blood was collected for analysis at 5-day intervals. Blood from healthy mice (receiving no inoculation) was also harvested and used as a control group. Forty microliters of blood was extracted from the tail and immediately mixed with anticoagulant. Whole blood was incubated with the fluorescent-conjugated antibodies anti-CD4-FITC and anti-CD8-PE (BD Biosciences) at 4°C for 30 minutes. Red blood cells were removed from the sample using a lysis buffer, Pharm Lyse (BD Biosciences). Lymphocytes were harvested after centrifugation at 500 rcf and washed 2 times with FACSflow. The pellet was resuspended in 200 μL FACSflow buffer and analyzed by FACSCalibur (BD Biosciences).

Statistical analysis

The differences in mean tumor size and percentage of T cells in blood from control and experimental mice were analyzed using Graphpad Prism 6.1 Software. P-values less than 0.05 were considered significant.

Results

Verapamil-resistant cells enriched stem cell populations

In groups with 10–40 μg/mL verapamil, cancer cells proliferated more slowly than in the control (0 μg/mL verapamil). Alternatively, at 60–100 μg/mL levels of verapamil, cancer cells were completely inhibited after 20 hours of treatment, and cell growth rates dramatically decreased and the cells died (Figure 1A). At 50 μg/mL verapamil, cancer cells were also inhibited after 20 hours of treatment, but there were a few living cells, so these populations continued to develop and formed verapamil-resistant cell populations. This concentration of verapamil was used to develop VRCs for the next experiment.

Figure 1 Selection of verapamil-resistant 4T1 cells. Notes: Effect of verapamil on the proliferation of 4T1 mouse mammary cancer cell line within 140 hours, with various verapamil concentrations (0–100 μg/mL) in RPMI-10% FBS medium at a density of 5,000 cells/well (A). The morphology of 4T1 cells before (B) and after (C) 48 hours of incubation in 50 μg/mL verapamil. Abbreviation: FBS, fetal bovine serum.

In the T-25 flask, 4T1 cancer cells were treated with 50 μg/mL verapamil in RPMI-10% FBS. There was a significant change in cell morphology and cell viability (Figure 1B). Cell membranes were not transparent, and the cells had a tendency to contract. Several 4T1 cells died and floated in the medium culture within 24 hours of exposure to verapamil, and the cell death ratio dramatically increased after 48 hours. Only the cells that could tolerate and resist verapamil survived and proliferated (Figure 1C).

ALDH expression in VRCs was analyzed. The results showed that these cells expressed ALDH (Figure 2A–C), and could form mammospheres in serum-free medium (Figure 2D). In the in vivo tumorigenesis assay, this population formed tumors with 10⁵ cells in mice (Figure 2E–G).

Figure 2 Verapamil-resistant cells exhibited stem cell phenotypes. Notes: Cells expressed ALDH in original 4T1 cells (A, B), and cells after selected by verapamil at 50 μg/mL (C). These VRCs also formed mammospheres in serum-free medium (D), and caused tumors with low doses of cells in mice (E–G). Arrows indicate the tumors. Abbreviations: VRCs, verapamil-resistant cells; SSC, side scatter; FSC, forward scatter.

Mesenchymal stem cells derived from murine bone marrow

After 24 hours of incubation, some mononuclear cells attached to the flask surfaces and exhibited the fibroblast-like shape (Figure 3H). These cells rapidly proliferated after 96 hours. These cells exhibited some properties of MSCs, such as positive expression of CD44, CD73, CD90, and CD105 (Figure 3D–G), but no expression of CD14, CD34, and CD45 (Figure 3A–C). These cells also successfully differentiated into adipocytes that stained with Oil red, and osteoblasts that stained with Alizarin red (Figure 3I, J). These cells continuously proliferated for five passages and were used for further experiments.

Figure 3 Mesenchymal stem cells isolated from bone marrow. Notes: These cells exhibited the mesenchymal stem cell particular phenotype such as negative with CD14, CD34, and CD45 (A–C), positive with CD44, CD73, CD90, and CD105 (D–G), fibroblast-like shape (H), successful differentiation into adipocytes that stained positive with Oil red staining (I), osteoblasts that stained positive with Alizarin red (J). Abbreviations: FITC, fluorescein isothiocyanate; PE, phycoerythrin; APC, allophycocyanin.

Production of functional dendritic cells from bone marrow-derived mononuclear cells with breast cancer stem cell and mesenchymal stem cell-derived antigens

Bone marrow-derived mononuclear cells were cultured in RPMI medium supplemented with GM-CSF and IL-4 for 7 days to generate immature DCs. Morphological observation on day 7 showed formation of dendrites that are typical of DCs (Figure 4A, B). On day 7, DCs still adhered to the culture flask bottom. These iDCs (immature dendritic cells) expressed the typical phenotypes of DCs, including the presence of CD80, CD86, and CD40 (Figure 4D–F) and the absence of CD14 (Figure 4C). Mature iDCs were induced by adding antigens into the culture medium with cytokines. After 3 days in the medium supplemented with antigens from both BCSCs and MSCs, DCs detached from the flask bottom and floated in the medium. Morphological observation showed that there are veils around the DCs.

Figure 4 Dendritic cells were generated from mouse bone marrow. Notes: Dendritic cells exhibited the particular morphology on day 5 in medium supplemented with GM-CSF and IL-4 (40× magnification) (A); on day 4 after induction by antigens (40× magnification) (B). The arrows indicate the dendrites on the DCs. Immune phenotype of DCs were characterized by flow cytometry (C–F). They expressed CD40 (D), CD86 (E), and CD80 (F) but lacked expression of CD14 (C). Abbreviations: DC, dendritic cells; GM-CSF, granulocyte-macrophage colony-stimulating factor.

Mouse bone marrow-derived DCs collected on day 10 of culturing (3 days after adding antigens) included populations of cells that expressed surface molecules that are typical for DCs. As shown in Figure 4C–F, the DCs expressed CD80 (94.42%), CD86 (87.41%), and CD40 (63.33%). The mouse bone marrow-derived DC populations expressed a few of the lineage markers for monocytes, including CD14 (2.65%). The DC populations generated in this study were mostly CD86, which is phenotypically characteristic of mature DCs, suggesting that mouse bone marrow cells cultured in a medium containing GM-CSF, IL-4 cytokine, and the antigens could successfully generate DCs that displayed typical DC surface antigens.

In vitro selective inhibition of breast cancer stem cell-dendritic cells and mesenchymal stem cell-dendritic cells on breast cancer stem cells

The results show that a mixture of DCs and CTLs effected BCSC proliferation that changed the CI (cell index) value recorded by the xCELLigence system (Figure 5). BCSCs normally proliferated over time in group 1. Group 2 demonstrated that a mixture of DCs and CTLs increased impedance slightly in the first 24 hours and was stable thereafter. From 0 to 24 hours (before adding CTLs), the proliferation rates in groups 1 and 3–6 were similar. After adding induced CTLs, from 24 to 63 hours, the effects of induced CTLs in all groups on BCSC proliferation were nonclear. However, from 63 to 98 hours, proliferation rates of groups 3–6 were somewhat different. BCSC proliferation in groups 3–6 was inhibited when a mixture of DCs and CTLs was added (Figure 5A).

Figure 5 In vitro selective inhibition of BCSC-DCs and MSC-DCs. Notes: BCSC-DCs and MSC-DCs incubated with CTLs at different ratios of DCs:CTLs suppressed BCSC proliferation and were measured by impedance using xCELLigence (A). Before adding CTLs, the cell proliferation rate in all groups was non-different from the control (B, D). After adding CTLs, MSC-DCs reduced proliferation rate compared with the control, while BCSC-DCs significantly inhibited BCSC proliferation at a DC:CTL ratio of 1:40 (C, E). Abbreviations: BCSC, breast cancer stem cells; CTL, cytotoxic T lymphocyte; DC, dendritic cells; MSC, mesenchymal stem cells.

Differences in ratios of DCs:CTLs also altered inhibition effects. Overall, there was increased BCSC inhibition in both the BCSC-DC and the MSC-DC groups with increased amounts of CTLs. When we compared the inhibition effects between the BCSC-DC and MSC-DC groups, we observed that although the DC-CTL mixture inhibited BCSC proliferation in both BCSC-DCs and MSC-DCs, BCSC-DC groups significantly decreased BCSC proliferation compared with MSC-DC (groups 5 and 6) groups and the control (group 1). There were also differences in inhibition of BCSC-DCs on BCSC proliferation at different ratios of DCs:CTLs, with the strongest inhibition occurring at a ratio of 1:40. These results are also supported by results from slope and doubling time analyses (Figure 5B–E).

In vivo selective inhibition of breast cancer stem cell-dendritic cells and mesenchymal stem cell-dendritic cells on tumors

Although there is no significant difference in daily tumor size between the 4 groups, we observed differences in increasing and decreasing tumor size between treated and control (RPMI 1640) groups (Figure 6A). On the basis of linear regression, the slopes of the control and the MSC-DC groups were positive, and the slopes of the BCSC-DC groups were negative (Figure 5B). This suggests that the tumor size of the groups treated with DCs primed by BCSC antigens decreased faster than that of those treated with DCs primed by MSC antigens and the control group. Slope values (Δy/Δx) were 0.003159±0.005604, 0.02555±0.004868, and −0.003324±0.005297 in the control, MSC-DC, and BCSC-DC groups, respectively. The slopes were significantly different (P=0.0001337).

Figure 6 Tumor growth in mice in three different groups. Notes: The tumor size decreased from 8 to 15 days; however, in the BCSC-DC group, tumor size reduced more rapidly than in the control (RPMI 1640) and MSC-DC groups. (A) Tumor sizes were measured day by day from day 2 to 14. (B) Linear regression analysis of the slope from day 2 to 15. Abbreviations: BCSC, breast cancer stem cells; DC, dendritic cells; MSC, mesenchymal stem cells.

The data can provide more evidence about changing tumor size when comparing tumor size between days 2 and 15 (Figure 7). Tumor size decreased 23% in the BCSC-DC groups. In contrast, tumor size increased 14% in the control group; in particular, in the MSC-DC group, tumor size increased 47%. This indicates that therapeutic treatment with DCs primed by BCSC-derived antigens is effective in decreasing tumor size. Moreover, DCs primed by MSC antigen actually caused tumor mass to increase.

Figure 7 Tumor mass harvested from mice on day 15. After sacrificing mice, tumors were collected by surgery. Notes: (A) Tumor from one mouse of control group where DCs were intravenously primed with MSC antigens (MSC-DC). (B) Tumors from all groups. Line I is from DCs intravenously primed with MSC antigens (MSC-DC), line II is from the control (RPMI 1640), line III is from DCs intravenously primed with BCSC antigen (BCSC-DC). The arrow indicates a tumor. Abbreviations: BCSC, breast cancer stem cells; DC, dendritic cells; MSC, mesenchymal stem cells.

T cell responses in mice after DC immunization

In order to elucidate the therapeutic effect of DCs on the immune system, mouse blood was harvested, and the percentage of CD4 and CD8 T cells was analyzed. Two days after inoculation with BCSCs, mice were injected with therapeutic DCs. Four days later, blood was harvested for evaluation. Assessment of lymphocytes was repeated 2 times, on days 7 and 13, after treatment. The results show that the amount of CD4 in normal mouse blood barely changed. However, there was a significant change in the treated groups. In mice with tumors that received no treatment (the control group), CD4 decreased by day 7 compared with day 4 (23% it decreased); in contrast, the amount of CD4 slightly increased, but nonsignificantly, in all of the DC-treated groups by day 7. By day 13, CD4 increased in both the non- and the DC-treated groups. In summary, the amount of CD4 in the nontreated group did not significantly increase over time (the start to the end of the experiment), but significantly increased in all of the DC-treated groups (P<0.05).

Similar to CD4, the amount of CD8 also changed in all mice. However, in contrast to CD4, the amount of CD8 increased by day 7. By day 13, the amount of CD8 significantly increased in treated groups compared with day 4 (P<0.05).

Discussion

Targeting cancer stem cells is considered an important approach in cancer treatment. However, the similarity between stem cells and cancer stem cells can cause mistargeting between stem cells and cancer stem cells, even though targeting cancer stem cells in glioblastoma was approved for clinical trial. Prior to this study, there was no comprehensive study that evaluated the cross-presentation of DCs between stem cells and cancer stem cells. In this study, we used BCSC and MSC models to investigate this concern, and MSCs from bone marrow were used because they are an important stem cell source in the body.

In the first step, BCSCs were enriched by the selection of verapamil-resistant 4T1 cells. In fact, one of the most common characteristics of cancer stem cells is anti-tumor drug resistance.^31–33 Thus, the anticancer drug assay is a functional assay that has been applied to enrich cancer stem cells.^34–36 This method is based on the overexpression of adenosine triphosphate-binding cassette (ABC) transporters on the membrane of cancer stem cells, such as P-glycoprotein (Pgp), multidrug resistance associated-protein 1 (MRP1), breast cancer resistance protein (BCRP), and multidrug resistance (MDR).

Recent studies have shown that increased expression of these transporters accounted for resistance of those cells to many anticancer drugs.³⁷ These ABC transporters play an important role in normal physiology by protecting cells from toxic xenobiotics and endogenous metabolites. Therefore, in high concentrations of anticancer drugs, overexpression of these ABC transporters could help drug-resistant cells pump drugs out of the cells, whereas normal cancer cells would die at such drug concentrations.

Verapamil, an anticancer drug, has been used as a drug target in many different types of cancer. In 1988, Huber et al³⁸ showed an antiproliferative effect of verapamil on growth rates of certain human brain tumor lines. Growth rates were inhibited by 10%–100% with 10–100 μM verapamil. Growth inhibition was accompanied by dose-dependent decreases in DNA, RNA, and protein synthesis that occurred within minutes after the addition of verapamil. A study by Trompier et al³⁹ demonstrated that verapamil behaves as an apoptogen or triggers apoptosis in MRP1-expressing cells after 8–16 hours of treatment. In this study, 50 μg/mL verapamil efficiently selected verapamil-resistant 4T1 cells; this was the maximum concentration of verapamil in which 4T1 could survive and grow. Our study reports, for the first time, the specific verapamil concentration necessary to develop drug-resistant cell populations in the 4T1 mouse mammary cancer cell line.

Overexpression of ABC superfamily multidrug efflux pumps is known to be responsible for chemoresistance.⁴⁰ These transporters play an important role in normal physiology by protecting cells from toxic xenobiotics and endogenous metabolites. Many clinically used drugs interact with the substrate-binding pocket of these proteins via flexible hydrophobic and hydrogen-bonding interactions. These efflux pumps are expressed in many human tumors, and expression combined with an enhanced capacity for DNA repair and decreased apoptosis contributes to resistance of tumor cells to chemotherapy treatment.⁴¹ Therefore, after allowing 48 hours of 4T1 cell exposure to a high concentration of verapamil (50 μg/mL), we expected that the viable remaining cells would overexpress ABC transporters and produce drug resistance.

Increased membrane transporter activity could help pump this anticancer drug out of the cells and lead to cell resistance at this drug concentration, whereas dead cells resulted from a lack of transporter activity. Consistent with this hypothesis, Calcagno et al³⁵ concluded that prolonged drug selection of breast cancer cell line MCF-7/ADR in doxorubicin could increase the cell population with stem cell characteristics. Thus, there was a high probability that a number of drug-resistant cells would be present in verapamil-treated cells. More importantly, verapamil-resistant 4T1 cells exhibited BCSC properties. These cells easily formed mammospheres in the serum-free medium, highly expressed ALDH, and caused tumors in both NOD/SCID and immune-deficient mice at low concentrations of cells. In fact, these properties were considered BCSC properties for a long time.^3,35,42–44 These verapamil-resistant 4T1 cells were considered BCSCs for this study.

Many studies have shown that DC therapy effectively inhibits breast cancer tumor growth,^23–25 indicating that DCs could specifically target BCSCs. In vitro assay demonstrated that BCSC-DCs induced CTLs that suppressed BCSC proliferation, while MSC-DCs induced CTLs that slightly suppressed BCSC proliferation. In fact, decreased proliferation rate of BCSCs treated with MSC-DCs induced CTLs related to nutrient competition in the medium owing to a high concentration of cells in these groups.

We also hypothesized that some MSC-DCs and induced CTLs could die and release granzyme and perforin that suppressed BCSC proliferation. This result was supported by in vivo assay. The data showed that treatment with DCs primed by BCSCs effectively suppress BCSC proliferation in breast tumor-bearing mice. We provided evidence that treating with BCSC-DCs by intravenous injection reduced initial tumor mass by 18%–23%. Conversely, tumors increased by 14% with no DC treatment. The effect of DC treatment was consistent with studies of DC treatment in human systems^45–47 and mouse models.⁴⁸ Interestingly, treatment with DCs primed by allogeneic MSCs (MSC-DCs) increased tumor size up to 47%. This means that immune response to reduce breast tumor did not occur when mice were treated with MSC-DCs.

In this study, besides the reduction of tumor size in the treated groups, the control group also showed decreasing tumor size. This finding is a little different from those of studies that used a more common breast tumor model.^48–50 This study used Swiss and mammary tumor 4T1 cell lines to develop a breast tumor model. The 4T1 cell line comes from BALB/c mice, whereas the Swiss mice retained the complete immune system. Therefore, mice would develop an immune response to the graft 4T1 cells, causing reduction of tumor size without any treatments. This may explain the reduction of tumor size in the control group on days 8–9. In treated mice, therapeutic DCs enhanced the immune system, causing a stronger reduction of tumor size. The lymphocyte data from blood after treatment provides more evidence for the effectiveness of DC therapy.

In the control group, there was no significant change in the amount of CD4 by day 7, but there was a significant increase in the amount of CD4 by day 13. This is consistent with the result of reduction of tumor size, which started to shrink by days 8–9 but not before day 7. This demonstrated that after day 7, the amount of CD4 T cells increased and there was efficient tumor reduction. However, the effect is not equal among all the groups. In the nontreated group, the amount of CD4 did not significantly increase by day 13, but there was a significant increase in the groups treated with MSC-DCs and BCSC-DCs by day 13 (P<0.05). Interestingly, although CD4 was high in all of the treated groups, the efficacy in tumor reduction occurred only in groups injected with BCSC-DCs and not MSC-DCs. We found little difference in the amount of CD8 between days 4 and 7 in all groups with tumor-carrying mice. These results show that BCSC-DCs, but not MSC-DCs, could induce immune response that targets tumors. Additionally, consistent with the results of studies that reported that therapeutic DCs enhance and support the response of CD4 T cells, CD8 T cells also kill cancer cells.^51,52

It is unclear why treatment with intravenous MSC-DCs caused tumor sizes to increase up to 47%, particularly compared with the BCSC-DC-treated groups. This increase could be caused by MSC-DCs inducing a large amount of immune cells specific to MSCs; therefore, the immune system weakly attacks breast tumor cells, thus facilitating tumor growth. More experiments with DCs primed by other cell lines are needed to understand this finding.

Conclusion

Cancer stem cells in tumors represent cell populations that can cause failure of chemotherapy as a cancer treatment. Targeting cancer stem cells is considered a promising therapy in cancer treatment. This study evaluated the specificity of DC therapy for targeting BCSCs in murine models. Both in vitro and in vivo DCs primed with BCSC-derived antigens inhibited BCSC proliferation in a target cell-specific manner. Although this study is limited by using a Swiss mouse model, therapeutic DCs clearly inhibit tumor size in a specific manner compared with the control group. These results support the application of DC therapy in targeting BCSCs as well as cancer stem cells.

Acknowledgment

This work was funded by a grant from the Ministry of Science and Technology, Vietnam (grant number DTDL.2011-T/30).

Disclosure

The authors report no conflicts of interest in this work.

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