Introduction
Recent antitumor drug research has seen the development of a large variety of antiangiogenesis therapies. Because cancer cells in tumors require new blood vessels to grow and spread, they stimulate capillary sprouting from existing vessels and new vessel formation from endothelial precursor cells [
1‐
4]. Recent clinical data shows benefit from the combined administration of antiangiogenic and cytotoxic (chemo- and radiation) therapies, because such combinations target two separate compartments of tumor cancer and endothelial cells. However, recent studies show that antiangiogenic agents also have a direct effect on tumor cells [
5,
6]. It is also the case that the cytotoxic agents used in chemo- and radiotherapy also affect endothelial cells and inhibit angiogenesis vice versa [
7‐
9].
Drug resistance is an obstacle that impairs the success of cancer therapies. In some cases relapse occurs in initially responsive patients after repeated cycles of chemotherapy due to the acquisition of tumor resistance [
10]. Multiple mechanisms contribute to drug resistance, such as increased drug efflux, altered drug metabolism, secondary mutations in drug targets, and the activation of downstream or parallel signal transduction pathways [
11,
12]. The critical mechanism of cell drug resistance involves the ABC (ATP-binding cassette) protein transporters which pump drug molecules out of cells, leading to reduced effective concentration within them [
13]. Well-known ABC transporters include the multidrug resistance (MDR) protein or P-glycoprotein (MDR1, P-gp, ABCB1); the multidrug resistance-associated proteins (MRP1, ABCC1); and the breast cancer resistance proteins (BCRP, ABCG2) [
14,
15].
P-gp is the first protein to have been shown to be involved in the MDR phenomenon and to be overexpressed primarily in cancer cells [
16,
17]. It is a protein of 170 kDa containing 1280 amino acids (aa) organized into 12 putative transmembrane domains shared out among two adenosine triphosphate (ATP)-binding cassettes [
18,
19]. Its role is well established in hepatic drug excretion and limitation of the gastrointestinal absorption of substrate drugs, and as a key component of the blood–brain, blood-testicular, and blood-placental barriers [
13,
20‐
24]. It is also expressed in circulating cells such as CD34
+ hematopoietic progenitor, CD8
+T cells or natural killer cells [
25]. Upregulation of P-gp has previously been shown to increase cancer cells’ ability to efflux a wide variety of structurally unrelated chemotherapeutics such as Vinca alkaloids (Vincristine, Vinblastine), Anthracyclins (Doxorubicin [Dox], Daunorubicin), and Epipodophyllotoxins (Etoposide) [
26‐
28]. Like P-gp, MRP1 and ABCG2 also have wide broad-substrate specificity [
29]. All three molecules are reported as being expressed in endothelial cells [
30‐
35].
Several published observations report high level expression of P-gp in tumor endothelial cells [
36,
37]. In this study, we characterize the induction of a major ABC protein in Human micro vessel endothelial cells (HMEC-1) and human umbilical vein endothelial cells (HUVEC) in response to long-term Doxorubicin treatment. The functional tests are then used to evaluate the protein function. Finally, the athymic mice are treated with Dox to observe the possible occurrence of induced drug resistance in mouse vessels. Our results suggest that P-gp overexpression in endothelial cells could be an early event in the development of chemoresistance and may contribute to the resistant phenotype of tumors
in vivo. This observation may be helpful when designing novel therapeutic strategies to improve cancer outcomes.
Materials and methods
Material
Mouse monoclonal antibodies against human P-gp: C219 were obtained from Calbiochem, La Jolla, CA; 4E3 from Dako, Glostrup, Denmark; and 265/F4 from Abcam, Paris, France. Antibody MRK16 blocking P-gp function was obtained from Kamiya Biomedical Company (Seattle, WA). The anti-ABCG2 antibody BXP-21 came from Abcam and the anti-MRP1 antibody QCRL-1 from Santa Cruz Biotechnology Inc., CA. The antibodies against vWF, flt-1, CD31, or CD105 as well as the FITC or HRP-conjugated F (ab’)
2
fragment of goat anti-mouse IgG were all provided by Dako. Doxorubicin chlorhydrate was purchased from Amersham Pharmacia Biotech (Uppsala, Sweden). Rhodamine 123 and Verapamil were obtained from Calbiochem and Daunorubicin, Etoposide, Vinblastine, Cyclosporine A, Fumitremorgin C, and Diethylstibesterol Terfenadine were provided by Sigma Chemical Co. (Saint Louis, MO).
Cell culture
Parental and resistant HMEC-1 (Dr TL Lawley, Department of Dermatology, Atlanta) lines were cultured in MCDB-131 medium supplemented with 10% fetal calf serum (FCS), 2 mM L-glutamine, 10 ng/ml EGF, 1 μg/ml hydrocortisone, 100 units/ml penicillin, and 100 μg/ml streptomycin as described elsewhere [
38]. Dox-resistant HMEC cells were obtained by continuously exposing cells to escalating concentrations of Dox from 0.001 μg/ml to 0.24 μg/ml over a 12-week period. Two subcell lines of HMEC-1 cells were collected: one was maintained in a culture with 0.08 μg/ml Dox (HMECd1 cells), and another with 0.24 μg/ml Dox (HMECd2 cells). No mutagenic agents were used in the establishment of these Dox-resistant HMEC cells. In the experiments looking at the reversibility of Dox resistance, both HMECd1 and HMECd2 cell lines were cultured in complete medium without Dox for four weeks. HUVEC were isolated as reported elsewhere [
39] and seeded on a 1% gelatin-coated plastic flask in MEM-199 medium supplemented with 20% FCS, 15 mM sodium bicarbonate, 15 mM hepes, 2 mM L-glutamine, 10 ng/ml EGF, 1 μg/ml hydrocortisone, 100 units/ml penicillin, and 100 μg/ml streptomycin. Human breast adenocarcinoma cells MDA-MB-435 were cultured in DMEM medium containing 10% FCS, 2 mM sodium pyruvate, 1 mM L-glutamine, 100 units/ml penicillin, and 100 μg/ml streptomycin. All types of cells were digested with trypsin-EDTA once or twice a week and cultured in a 37°C incubator with a 100% humidified atmosphere of 5% CO
2.
3H-thymidine Cell proliferation assay
Parental and resistant HMEC sublines were seeded at a density of 4 x 104 cells per well in 48-well culture plates and exposed to a range of drug concentrations for 72 hours at 37°C in an atmosphere of 5% CO2. After 70 hours incubation, 1 μCi 3H-thymidine (Amersham Pharmacia biotech) was added per well for 2 hours. Wells were then washed twice in PBS and successively incubated with 5% trichloroacetic acid for 20 minutes at 4°C and then 0.5 N NaOH for 90 minutes at 37°C. Radioactivity incorporated into adherent cells was recorded on a β counter (Beckman). The 50% cytotoxic concentration (IC50) values were defined as the drug concentration producing 50% inhibition of cell growth and the resistance index (RI) corresponded to the ratio of IC50 values between the resistant and parental cell lines.
MTS cell proliferation assay
Cell viability was determined using the MTS cell proliferation assay (Promega). Cells grew to a confluence of 90% in 75 cm2 cell culture flasks and were passed into 96-well plates (7500 cells/well). Each well contained 100 μl of culture medium supplemented with various concentrations of drugs or with a concentration of DMSO as control. After incubation for either 24, 48, or 72 hours, 20 μl of the MTS reagent was added to each well, and the plate placed in the 5% CO2 incubator at 37°C for an additional 2 hours. The optical density (OD) was then read at 492 nm using a microplate reader (Labsystems Multiskan MS). The IC50 values were defined as the concentration of drug producing 50% inhibition of cell growth and the RI corresponded to the ratio of IC50 values between the resistant and parental cell lines. Experiments were performed in triplicate and repeated at least three times.
Blocking effect assay
P-gp inhibitors Cyclosporine A at 2.5 μM or Verapamil at 1 μM and ABCG2 inhibitors Fumitremorgin C at 5 μM or Diethylstibesterol at 0.5 μM were used in these experiments. After incubation for 48 or 72 hours, cell viability was assessed by the MTS assay. The reversal fold (RF) values, as a measure of the potency of reversal, were obtained from fitting the data to RF = IC50 of cytotoxic drug alone/IC50 of cytotoxic drug in the presence of a modulator [
40].
Rhodamine-123 (Rho) accumulation and efflux assay
HMEC-1, HMECd1, and HMECd2 cells (106/ml in PBS-BSA) were incubated with 1–2 μg/ml Rho in the dark at 37°C in 5% CO2 for one hour. Then, the cells were washed twice with ice-cold PBS and analyzed immediately using flow cytometry at different time points. To test Rho efflux specificity, cells were incubated with 30 μM Verapamil or 10 μg/ml MRK16. Results were expressed in an arbitrary unit of the mean fluorescence intensity (MFI). The drug efflux was expressed relative to the amount of drug accumulated.
Evaluation of mRNA expression via qPCR
HMEC-1, HMECd1, and HMECd2 cells were treated with 2.5 μM Cyclosporine A, 1 μM Verapamil, 5 μM Fumitremorgin C, or 0.5 μM Diethylstibesterol for 24 hours. After incubation, the treated and non-treated cells were harvested and total RNA prepared using the SV total RNA isolation system kit (Promega, USA). The purity of total RNA was checked by a ratio of A260/A280 (>1.9). Total RNA (50 ng) was used to synthesize the first-strand cDNA in a 20 μl reaction solution using the GoScript Reverse Transcription System kit (Promega, USA). Then, 2 μl of cDNA was used for qPCR in triplicates using a taqman® gene expression assay, the primers for P-gp (Hs01067802_m1), ABCG2 (Hs01053790_m1), and the primers for TBP as controls (TATA box binding protein, Hs99999910_m1, Applied Biosystem). The qPCR was performed by 10 minutes of initial denaturation followed by 44 cycles of 15 s at 95°C and 60 s at 60°C in a BioRad CFX96® Real-time System. Delta Ct method was used for analyzing the qPCR results and TBP was used as an internal control for mRNA-level normalization.
Evaluation of protein expression using western blot analysis
Western blot was performed on whole cell lysates by incubating the cells in the lysis buffer (10 mM Tris pH 6.8, 1 mM EDTA, 10% NP40, 1 mM PMSF, 0.1% SDS) on ice for 30 minutes. Cell debris was removed by centrifugation at 16000 g for 10 minutes. Protein concentration was determined by BCA™ protein assay (Thermo Scientific, USA). A 50 μg protein of each sample was loaded on 8% SDS-PAGE, and the protein transferred to a PVDF membrane by the iBlot™ dry blotting system (Invitrogen, USA). The membranes were blocked by 5% nonfat dry milk for one hour and incubated with either anti-P-gp (Abcam ab-3364) or anti-ABCG2 antibodies (Abcam ab-3380) at 4°C overnight. They were then washed with TBS-tween buffer for one hour and incubated with appropriate HRP-conjugated secondary antibodies (Invitrogen Corp) diluted in blocking buffer for one hour at room temperature. After washing, western blotting luminol reagent (Santa Cruz Biotechnology, USA) was added to the membranes and the chemiluminescence recorded using a Fuji LAS-3000 system. The membranes were then treated with antibody stripping buffer (Gene Bio-application Ltd. Israel), and incubated with anti-actin antibody (1:4000 dilution, Sigma, USA) as control.
In vivo assays
Mice were maintained under specific pathogen-free conditions in the animal facility of the Institut Universitaire d’Hématologie, Saint Louis Hospital in Paris. All experimental procedures were performed in accordance with the recommendations of the European Community (86/609/EEC) and the French National Committee (87/848) for the care and use of laboratory animals. Female athymic nude mice Nu/Nu Swiss (9 weeks of age) (Iffa-credo, France), weighing 18–22 g, were housed under controlled environmental conditions (approximately 25°C) with commercial food and water freely available. Primary results showed that the maximal tolerated dose of Dox by athymic mice for a 6 week period was 6 mg/kg/week. Dox was prepared in 0.9% sodium chloride and ip injections given twice weekly. The experimental procedure consisted of a pretreatment of the mice for 15 days with sodium chloride as a control or 6 mg/kg/week Dox. MDA-MB-435 cells (4×106 cells/200 μl PBS) were then injected subcutaneously into their dorsal midline. Tumor growth was determined 25 days after cell injection and sizes monitored by measuring two diameters with a dial-caliper. Tumor volume was calculated as TV = length × (width)2 × π/6.
At the end of the experiments, the mice were sacrificed and the percentage of endothelial cells expressing P-gp on the liver, kidneys, heart, and tumor measured by flow cytometry. Tissues were cut into approximately 1×1-mm2 squares and rinsed in physiologic serum. The pieces were incubated with 2 mg/ml collagenase at 37°C for 20 minutes with frequent agitation. The cell suspension obtained following extensive trituration with a 5 ml pipette was filtered on a 70 μm nylon cell strainer followed by a second 40 μm filtration. The second filtrates were centrifuged at 1200 rpm for 5 minutes and the pellets washed twice in 1 ml PBS containing 0.5% BSA. Endothelial cells were isolated by immunoabsorption on magnetic beads coated with anti-mouse CD31 and CD105 IgG according to the recommended protocol (Myltenyi Biotec, France). The isolated cells were characterized by flow cytometry using anti-mouse vWF IgG or C219 antibody. Labeling was revealed by second incubation with fluorescein-conjugated goat anti-mouse IgG.
Immunohistochemical staining
Immunohistochemical studies were carried out on 5 μm paraffin sections before and after treatment. Primary antibody against P-gp C219 antibody was used at 1:50 dilution. All the immunostainings were performed in an automated immunostainer (Ventana Medical System, France). The intensity and percentage of the cytoplasmic staining on tumor sections were noted.
Statistical analyses
Data were analyzed using one-way ANOVA and Mann–Whitney U tests as appropriate. The data of qPCR, invasion assay, and in vivo data are presented as mean ± SEM. The rest of the data is presented as mean ± SD. A probability value of ≤ 0.05 was regarded as statistically significant.
Discussion
This study was designed to evaluate the expression of P-gp, MRP1, and ABCG2 and their activities in endothelial cells after cell exposure to Dox. We have shown for the first time that P-gp expression was upregulated in two stabilized Dox-resistant endothelial cells, HMECd1 and HMECd2. P-gp protein levels revealed by western blots were found to have increased 4- and 6- fold in both HMECd1 and HMECd2 cells. Similarly, the qPCR experiment demonstrated 3.4 and 7.2 fold increases in P-gp gene expression. The functional efflux test using Rho 123 demonstrates a linear correlation between P-gp transporter expression and efflux function. We further show that the drug spectrum of P-gp-mediated drug resistance corresponded to the P-gp functional character and that the blockage of P-gp activity by the P-gp inhibitors Verapamil and Cyclosporine A attenuated the cells’ capacity for Dox resistance. Furthermore, we demonstrate that the resistant cell phonotype induced by Dox treatment can be slowly reversed after withdrawal of the drug in culture.
We studied ABCG2 because it is another well-known ABC transporter used to efflux a wide variety of substrates, in particular some anticancer drugs such as Mitoxantrone, Doxorubicin, and Daunorubicin [
29,
41]. We observed a significant induction of ABCG2 expression in HMECd1 and HMECd2, though this was much less pronounced than that of P-gp. Since both inhibitors of ABCG2 (Fumitremorgin C and Diethylstibesterol) failed to reverse Dox resistance in HMECd1 and HMECd2, this also suggests that the drug efflux in HMECd1 and HMECd2 was due to the upregulated P-gp level. MRP1 was also evaluated in this study. However, neither western blot nor flow cytometry detected its significant expression in noninduced cells nor was there an increase in expression in the induced cells. Accordingly, the anti-MRP1 antibody QCRL-1 MoAb had no effect on cell survival. Although ABCG2 and MRP1 were shown not to be functionally responsible for the drug resistance observed here, the possibility that they may play important roles in the drug resistance of endothelial cells in other circumstances cannot be excluded [
34,
35,
42].
Recent studies have emphasized the importance of tumor vasculature and an appropriate pressure gradient for adequate drug delivery to the tumor [
43‐
45]. In addition, some cancer cells that are sensitive to chemotherapy in cultured cell monolayers become resistant when transplanted into animal models. This indicates that environmental factors such as the extracellular matrix or tumor geometry might be involved in tumor drug resistance [
46].
Our data also give rise to questions about the involvement of acquired P-gp expression on endothelial cells in tumor resistance. To induce P-gp upregulation, we firstly treated the mice with Dox before tumor implantation. The results of the immunostaining and cytometry analysis of the isolation of endothelial cells shown in Figure
3 demonstrate significantly higher P-gp expression in the livers and kidneys of the treated mice, confirming the rapid response of normal endothelial cells to Dox challenge. These observations are in agreement with the tissue distribution of P-gp [
47]. We further isolated the endothelial cells from the tumors, and the results clearly demonstrated a higher expression of P-gp on the tumor vessels after Dox treatment. The highest expression of P-gp was found in those mice that had been treated with Dox before tumor implantation, whereas positive, but less stained, endothelial cells were observed in the short treatment groups, compared to the negative control mice. Immunochemical staining of the tumor sections confirmed the result. These results indicate that normal vessels as well as tumor vessels react to Dox injection. Our results are also consistent with recent studies showing that endothelial cells isolated from human tumors are less sensitive to anticancer drugs [
28,
48].
To evaluate the effect of the acquired Dox resistance of endothelial cells on tumor growth in preclinical models, we also evaluated tumor growth in the mice where such resistance had been induced. The results demonstrated that Dox has an inhibitory effect on MDA-MB-435 tumor growth transplanted into control nude mice. In the mice that had been pretreated by Dox before tumor graft, tumor growth continued and responded poorly to Dox treatment. Acquired resistance to Dox in the pretreated group is believed to greatly reduce the anti-cancer efficacy of Dox. Importantly, as demonstrated in this model by P-gp immune staining of the tumor sections, upregulation of P-gp expression after Dox treatment was found essentially in tumor endothelial cells, but not in tumor cells themselves. Therefore, these results strongly suggest that acquired resistance in tumor endothelial cells plays a role in the overall therapeutic response to anticancer drugs.
Taken together, these findings underline the importance of drug resistance in endothelial cells in both
in vitro and
in vivo experiments. Recent reports provided evidence for acquired drug resistance in tumor endothelial cells in cancer patients [
36,
37]. We believe that further investigation of this aspect will be helpful in understanding the complex mechanisms of MDR in cancer. We hope that circumventing endothelial cell drug resistance may improve conventional chemo- and antiangiogenic therapies.
Acknowledgements
We thank the institute of cancer (INCA, PL06_130), the Association pour la Recherche sur le Cancer (ARC); the Ligue Nationale contre le Cancer (Ligue), the Fondation de France, and the Association Ti’toine for their support. We are grateful to Prs L Cazin and JP Vannier for their support.
Competing interests
The authors declare that they have no competing interests.