Caveolin-1 (Cav-1), the major component of caveolae, is a 21–24 kDa integral membrane protein that interacts with a number of signaling molecules. By acting as a scaffolding protein, Cav-1 plays crucial roles in the regulation of various physiologic and patho-physiologic processes including oncogenic transformation and tumorigenesis, and tumor invasion and metastasis.
In the present study we sought to explore the role of Cav-1 in response to DNA damage and the mechanism involved. We found that the level of Cav-1 was up-regulated rapidly in cells treated with ionizing radiation. The up-regulation of Cav-1 following DNA damage occurred only in cells expressing endogenous Cav-1, and was associated with the activation of DNA damage response pathways. Furthermore, we demonstrated that the expression of Cav-1 protected cells against DNA damage through modulating the activities of both the homologous recombination (HR) and non-homologous end joining (NHEJ) repair systems, as evidenced by the inhibitory effects of the Cav-1-targeted siRNA on cell survival, HR frequency, phosphorylation of DNA-dependent protein kinase (DNA-PK), and nuclear translocation of epidermal growth factor receptor (EGFR) following DNA damage, and by the stimulatory effect of the forced expression of Cav-1 on NHEJ frequency.
Our results indicate that Cav-1 may play a critical role in sensing genotoxic stress and in orchestrating the response of cells to DNA damage through regulating the important molecules involved in maintaining genomic integrity.
Citation: Zhu H, Yue J, Pan Z, Wu H, Cheng Y, Lu H, et al. (2010) Involvement of Caveolin-1 in Repair of DNA Damage through Both Homologous Recombination and Non-Homologous End Joining. PLoS ONE 5(8): e12055. doi:10.1371/journal.pone.0012055
Editor: Mark R. Cookson, National Institutes of Health, United States of America
Received: March 10, 2010; Accepted: July 12, 2010; Published: August 6, 2010
Copyright: © 2010 Zhu et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by grants from the National Cancer Institute CA109371 (Yang), CA066077 (Yang) and CA137738 (Shen). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Caveolin-1 (Cav-1), a major structural protein of caveolae, is involved in many physiologic and patho-physiologic processes such as cardiovascular diseases, neurological disorders, and cancers. Although accumulating evidence indicate that expression of Cav-1 is altered in a stage-dependent manner during progression of various types of cancers , , , , the precise roles of Cav-1 in cancer development, progression, and treatment remain to be fully defined. Based on its location at chromosome 7 (7q31.1), which is frequently deleted in human malignancies , Cav-1 is believed to be a tumor suppressor. Indeed, Cav-1 was found to be down-regulated in many types of cancers including breast cancer , colon cancer , lung cancer , , , ovarian cancer , , sarcomas , and thyroid cancer . Forced expression of Cav-1 inhibits tumor growth and induces apoptosis of tumor cells , . Additionally, a mutation in Cav-1 at codon 132 (P132L) was found in 16% of the primary human breast cancer cases , and interbreeding Cav1−/− mice with MMTVPyMT mice (mouse mammary tumor virus-Polyoma middle T antigen) accelerated onset of mammary tumors in their offspring .
On the other hand, up-regulation of Cav-1 has been observed in highly metastatic human cancers, and is associated with poor clinical prognosis , , , , , , , , , , , ,  and with resistance to therapy , . These observations indicate that re-expression of Cav-1 at advanced stages of cancer may play a pro-survival role that protects tumor cells against various stresses such as micro-environmental and therapeutic stress. Recently, it was demonstrated that expression of Cav-1 promotes survival of cancer cells following treatment with ionizing radiation (IR) , , further supporting Cav-1 as a stress protector in malignant cells. The protective effect of Cav-1 on IR-treated cells also suggests that this signaling-modulating molecule may play an important role in repair of damaged DNA. The main DNA damage caused by IR is double strand break (DSB), which can be repaired by two major pathways: homologous recombination (HR) and non-homologous end joining (NHEJ). HR pathway can accurately repair DSB via exchange of genetic material between two similar or identical strands of DNA; NHEJ is a repairing process in which the break ends are directly ligated without the need for a homologous template and thus is error-prone. As damage of DNA not only causes neoplasm but is also utilized in therapeutic interventions such as radiotherapy and chemotherapy, and as Cav-1 is differentially expressed during tumor progression, understanding the role of Cav-1 in DNA DSB repair and the underlying mechanism(s) may help further decipher the signaling pathways involved in tumor initiation and progression, and help develop new approaches to the prevention and treatment of cancers. We report here that the up-regulation of Cav-1 protein in response to DNA damage plays an important role in activating DNA repair signaling cascade and in promoting repair of DSB through both HR and NHEJ, thus contributing to maintenance of genomic integrity.
Genotoxic stress induces a transcriptionally independent up-regulation of Cav-1
Expression of Cav-1 was reported to be elevated in cells exposed to IR , . As shown in Fig. 1A, treatment with IR stimulated the expression of Cav-1 protein in MDA-MB-468 cells. The DNA damage-induced Cav-1 up-regulation also occurred in other cell lines (both tumor cells and non-tumor cells) expressing endogenous Cav-1 such as NCI/ADR-RES, T98G and MCF-10A, but not in cell lines (MCF-7 and PC-3) that do not express endogenous Cav-1 (Fig. 1B), and did not appear to result from altered transcription of the Cav-1 gene, because IR did not affect the level of Cav-1 mRNA in MDA-MB-468 and A549 cells with or without silencing of Cav-1, as determined by qRT-PCR (Fig. 2). With the use of these cell lines containing different status of p53, it appeared that IR – induced alteration of Cav-1 was independent of p53 status.
(A) MDA-MB-468 cells were irradiated (5 Gy) for the indicated period of time, and then the treated cells were collected for Western blot analysis of Cav-1. β-actin was used as a loading control. Expression of Cav-1 and β-actin were quantified using imageJ software, and Cav-1 level was normalized to that of β-actin. The normalized Cav-1 at the zero time point was arbitrarily set as 1. Bar represent mean ± S.D. of three separate experiments. (B) MCF-7, NCI/ADR-RES, PC-3, T98G and MCF-10A cells were treated or untreated with 5 Gy ionizing radiation, and Cav-1 expression was analyzed by Western blot. Results shown are the representative of three identical experiments.
MDA-MB-468 and A549 cells were transfected with a non-targeting RNA or siRNA against Cav-1. Twenty-four hours later, cells were treated with 5 Gy radiation for the indicated period of time. To determine Cav-1 mRNA, total RNAs were extracted from the cells and quantitative real-time RT-PCR was performed. Cav-1 mRNA level was normalized to β-actin mRNA. The Cav-1 mRNA level of the cells treated with the non-targeting RNA and without IR treatment was arbitrarily set as 1. Results shown are the representative of three similar experiments; each bar represents mean ± SD of quadruplicate determinations.
Expression of Cav-1 is associated with DNA damage response pathways
To further define the roles Cav-1 in DNA damage response, we examined the effects of Cav-1 on signaling pathways that participate in DNA repair. siRNAs were utilized to inhibit Cav-1 expression. To avoid “off-target” effects of siRNA, we used two Cav-1-targeted siRNA sequences that both knocked down Cav-1 expression (Fig. 3A). We found that IR - induced accumulation of single-strand DNA (ssDNA) was increased in the cells transfected with the Cav-1-targeted siRNA, as compared to the cells transfected with a non - targeting RNA (Fig. 3B). The levels of γ-H2AX, the phosphorylated form of H2AX (at Ser139) associated with DSB, were also significantly higher in MDA-MB-468 cells with silencing of Cav-1 expression than in cells treated with a non-targeting RNA following IR (Fig. 3C), another evidence for defective DNA repair caused by loss of Cav-1. These observations suggest that Cav-1 defect may impair DNA damage repair.
(A) MDA-MB-468 cells were transfected with a non-targeting RNA (NT) or either Cav-1-targeted siRNA sequence 1 or sequence 2. At the indicated time following transfection, the cells were collected for Western blot analysis of Cav-1. β-actin was used as a loading control. (B) MDA-MB-468 cells were transfected with a Cav-1 siRNA or a non-targeting RNA, followed by IR (5 Gy). The cells were collected at the indicated time points and fixed for immunofluorescent detection of ssDNA. The signals of ssDNA and total DNA were quantified using imageJ software, and ssDNA signal was normalized to total DNA signal at each time point. The results shown were mean±S.E. of five similar experiments. * p<0.05; ** p<0.01. (C) MDA-MB-468 cells were transfected with a Cav-1-targeted siRNA or a non-targeting control (NT). Forty-eight hours later, the transfected cells were irradiated (5 Gy) for the indicated period of time followed by Western blot analysis of γ-H2AX. Levels of γ-H2AX and H2AX were quantified using imageJ software. γ-H2AX/H2AX ratios of untreated samples (zero time) were arbitrarily set at 100 as controls, and the treated samples were normalized to the controls. Results shown are the representative of three similar experiments; each point represents mean ± SD of triplicate determinations. * p<0.05, ** p<0.01.
Furthermore, we investigated whether suppression of Cav-1 resulted in impairment of DNA damage signaling. As shown in Fig. 4A, the activity of ATM, a kinase that is activated by DNA damage signals and phosphorylates a series of downstream targets such as CHK2, was lower in the cells with silencing of Cav-1 than that in the control cells following IR, as demonstrated by decreased levels of the phospho-ATM (Ser1981) and phospho-CHK2 (Thr68). Treatment of cells with inhibitors (okadaic acid and calyculin A) of PP2A, a phosphatase that decreases ATM phosphorylation, augmented the IR-induced phosphorylation of ATM (Fig. 4B), indicating the involvement of PP2A in the regulation of ATM activity in response to DNA damage. Moreover, our co-immunoprecipitation experiments demonstrated an increased physical association between Cav-1 with PP2A following IR (Fig. 4C). These results suggest that in response to DNA damage, Cav-1 plays an essential role in activating the ATM-initiated repair pathway by sequestering and inhibiting the function of PP2A. Also, using immunofluorescent microscopy we observed that knockdown of Cav-1 by siRNA reduced both the spontaneous and IR-induced foci formation of BRCA1, a DNA repair protein whose expression is controlled by Cav-1 (Fig. 5). The reduction of BRCA1 foci did not appear to be a consequence of changes in cell cycle, as the silencing of Cav-1 had no effect on cell cycle distribution (Fig. 6). These observations provide additional evidence that depletion of Cav-1 weakens the ability of cells to repair damaged DNA.
(A) MDA-MB-468 cells were transfected with a Cav-1 siRNA or a non-targeting RNA, followed by IR (5Gy) for the indicated period of time. The treated cells were collected for Western blot analysis of phospho-ATM, total ATM, phospho-CHK2, and tubulin. (B) MDA-MB-468 cells were irradiated (5Gy) for the indicated period of time in the absence or presence of the PP2A inhibitors, okadaic acid or calyculin A. The treated cells were collected for Western blot analysis of phospho-ATM and total ATM. Tubulin was used as a loading control. In order to show changes of phosphor-ATM, the results of two exposures were included. LT: 1 min exposure; ST: 10 sec exposure. (C) MDA-MB-468 cells were irradiated (5 Gy) for the indicated period of time, followed by immunoprecipitation and immunoblotting with the indicated antibodies. The results shown are the representative of three similar experiments.
MDA-MB-468 cells were transfected with a Cav-1 siRNA or a non-targeting RNA. Forty-eight hours later, the cells were irradiated (5 Gy), and fixed for immunostaining with a BRCA1 antibody. BRCA1 foci were shown in green. DAPI was used for nucleus staining.
MDA-MB-468 cells with or without silencing of Cav-1 were fixed for cell cycle analysis by FACS at the indicated time following IR treatment. The results shown are the representative of three similar experiments; each bar represents the mean±S.D. of triplicate determinations.
Expression of Cav-1 is required for HR repair of damaged DNA
To begin to explore the mechanism by which Cav-1 regulates DNA repair, we first tested whether silencing of Cav-1 expression by siRNA altered the frequency of HR, one of the major pathways involved in DSB repair. We used HT1080 cell line and an HR reporter system developed by Brenneman et al . HT1080 cell line carries a single integrated copy of a puro direct repeat HR substrate. One of the puro repeats is driven by the PGK promoter, but is inactive due to the insertion of an I-SceI recognition site; the second allele codes the wild-type protein, but lacks a promoter (Fig. 7). Introduction of an I-SceI expression vector into HT1080 cells creates DSBs at the I-SceI site, and only repair of these DSBs by HR can produce a functional puro that confers puromycin resistance. Fig. 8A demonstrates that similar to other Cav-1-expressing cell lines, HT1080 cells showed an increased expression of Cav-1 following IR. To determine the effect of Cav-1 on HR, HT1080 cells were transfected with an I-SceI expression vector, selected with puromycin, and then treated with a Cav-1 siRNA or non-targeting RNA. In HT1080 cells, the silencing effect of Cav-1 siRNA could last until day 6 after transfection (Fig. 8B), which is within the timeframe required assaying HR. Fig. 8C shows that there was an equal level of I-SceI expression in Cav-1 knockdown and control cells, but the Cav-1 knockdown cells had significantly lower level of HR after I-SceI expression.
(A) HT-1080 cells were irradiated (5 Gy) for the indicated period of time, and then cell lysates were prepared for Western blot analysis of Cav-1 and γ-H2AX. β-actin was used as a loading control. (B) To determine the turnover of the silencing effect of Cav-1 siRNA in HT-1080 cells, we performed Western blot of analysis of Cav-1 at the indicated time after siRNA transfection. (C) HT-1080 cells were transfected with a non-targeting RNA or Cav-1 siRNA. Twenty-four hours after transfection, the cells were transfected with an HA tagged I-SceI endonuclease expressing vector (HA-I-SceI) or empty vector (HA) by electroporation, followed by Western blot analysis of Cav-1 and HA-I-SceI (upper panels), and by puromycin screening for HR frequency (lower panels). HR frequency was calculated as follows: the average numbers of colonies/dish were divided by the plating efficiency of transfection and divided by 85,000 (the total number of cells plated). The results shown are the representative of three similar experiments; each bar represents the mean±S.D. of triplicate determinations.
Expression of Cav-1 promotes NHEJ in response to DNA damage
NHEJ is another major pathway for mammalian cells to repair DSB . As shown above in Fig. 6, silencing of Cav-1 reduced the foci formation of BRCA1. As BRCA1 is a protein know to be involved in DSB signal transduction and may regulate both HR and NHEJ, we next wanted to know if Cav-1 is involved in the regulation of this important DNA repair pathway. The phosphorylation of DNA-PK, one of the necessary components of the NHEJ pathway, was used as a read-out of this repair system. We found that although exposure of MDA-MB-468 cells to IR markedly induced DNA-PK phosphorylation at Ser2056, suppression of Cav-1 expression by siRNA effectively inhibited the IR- stimulated phosphorylation of this critical DSB repair factor (Fig. 9A), suggesting that Cav-1 is involved in controlling the activity of the NHEJ pathway. The results of the NHEJ assay, which measures overall frequency of NHEJ , demonstrated that introduction of Cav-1 into HEK293 cells (Fig. 9B, left panel) significantly increased the NHEJ frequency as compared to the transfection with a control empty vector (a 40% increase was observed) (Fig. 9B, right panel). To further analyze how Cav-1 regulates the phosphorylation of DNA-PK, we examined the effect of Cav-1 on IR-induced nuclear translocation of EGFR, which is known to interact with DNA-PK and promote its phosphorylation . To further examine the localization of Cav-1 and EGFR in response to IR treatment, we immunostained the cells with Cav-1 (in green) and EGFR (in red) before and after IR treatment. As shown in Fig. 9C, Cav-1 and EGFR were located on plasma membrane before IR treatment, but co-translocations of Cav-1 and EGFR in the nuclei were observed 1 h following IR, as visualized by confocal microscopy. By contrast, the nuclear co-translocation of these two proteins was barely seen in the cells with silencing of Cav-1 (Fig. 9C). The similar intensity of Cav-1 staining in the cells transfected with a Cav-1 siRNA or a non-targeting RNA was likely due to the high affinity of the Cav-1 antibody and the high sensitivity of the immunofluorescence detection method. Physical association between Cav-1 and EGFR also increased following IR (Fig. 9D). These results suggest that Cav-1 can control NHEJ through modulating the activity of DNA-PK via Cav-1-mediated nuclear translocation of EGFR.
(A) MDA-MB-468 cells with or without silencing of Cav-1 were irradiated (5 Gy) for the indicated periods of time, and then subjected to Western blot analysis of phosphor-DNA-PKcs and total DNA-PKcs. (B) Left panel: HEK 293 cells containing a GFP-based chromosomal reporter, EJ5-GFP, were transfected with a caveolin-1 expression vector or a control empty vector. Thirty-six hours later, the cells were transfected with an HA tagged I-SceI endonuclease expression vector or an empty vector. Expressions of Cav-1 and HA-I-SceI were determined by Western blot. Right panel: Seventy-two hours following transfection with the HA-I-I-SceI plasmid, percentage of EGFP expressing cells, which represents the frequency of NHEJ, were determined by flow cytometry. The results shown are the mean ± S.E. from three identical experiments. (C) MDA-MB-468 cells with or without silencing of Cav-1were irradiated (5 Gy) for the indicated periods of time, and then fixed for immunostaining with Cav-1 and EGFR antibodies. Cav-1 staining was shown in green and EGFR staining in red. DAPI was used for nucleus staining. (D) MDA-MB-468 cells were irradiated (5 Gy) for the indicated periods of time. At the end of IR, cells lysates were prepared and subjected to immunoprecipitation and immunoblotting with either Cav-1 or EGFR antibodies as indicated. The light chain and heavy chains were used as loading controls.
Silencing of Cav-1 expression increases sensitivity of cancer cells to genotoxic stresses
To assess the functional significance of the up-regulation of Cav-1 in response to DNA damage, we examined the effect of silencing of Cav-1 expression on survival of the cells treated with IR, using a colony formation assay. Fig. 10 shows that IR caused a significantly more killing in the cells with loss of Cav-1 than in the control cells, further supporting a role of Cav-1 in protecting cells against genotoxic stress.
MDA-MB-468 cells with or without silencing of Cav-1 were treated with varying doses of γ-radiation, and colony formation assay was performed to compare cell survival. Results shown are the representative of three similar experiments; each point represents mean ± SD of quadruplicate determinations of the experiment.
Loss of the putative tumor suppressor, Cav-1, is believed to be one of the causes for development of several types of cancers, but evidence also show that overexpression or re-expression of Cav-1 in advanced stages of the disease may contribute to tumor progression. Yet, how loss of Cav-1 facilitates tumorigenesis and how re-induction of Cav-1 promotes tumor progression remain an open question. It has been reported that expression of Cav-1 favors cancer cell proliferation by regulating survival pathways such as Rac, Erk and PtdIns 3-kinase  and inhibits detachment-induced apoptosis (anoikis) either through suppressing p53 activation  or up-regulating the transcription of the IGF-I receptor gene . We previously demonstrated that Cav-1- regulated calcium homeostasis plays a role in growth and survival of breast cancer cells . In the present study, we sought to determine the functional significance of Cav-1 up-regulation caused by treatments with DNA damaging agents, a phenomenon that was also observed by others , , . Our study reveals a new function of Cav-1 as a possible sensor and mediator in the DNA damage response/repair process. We show that expression of Cav-1 can be rapidly up-regulated by DNA damaging agents such as IR (Fig. 1), and that the up-regulation of Cav-1 protein plays a critical role in activating the DNA repair signaling cascade, since depletion of Cav-1 expression by siRNA impairs the cells' ability to repair DNA, as evidenced by increased accumulation of g-H2AX (Fig. 3C) and ssDNA (Fig. 3B), reduced phosphorylation of ATM at Ser1981 and CHK2 at Thr68 (Fig. 4A), and decreased formation of BRCA1 foci (Fig. 5). Moreover, our study reveals for the first time that Cav-1 is able to regulate both HR and NHEJ pathways, two major mechanisms responsible for repair of DNA DSB. This conclusion is supported by use of two assays specific for detecting HR and NHEJ. In the current study, the repair of DSBs induced by the I-SceI endonuclease is monitored using artificial chromosome-integrated reporters, namely HT1080-1885 for HR pathway (Fig. 8) and EJ5-GFP for NHEJ pathway (Fig. 9). Each individual reporter is designed such that repair of I-SceI-induced DSBs by a specific pathway restores a puromycin resistance or a GFP expression cassette. In each of the reporter-containing cell lines, the activation of the reporter is confirmed to be dependent upon expression of I-SceI. The restoration of puromycin resistance in HT1080-1885 can only be achieved by HR repair of I-SceI induced DSB using downstream homologue as template. For EJ5-GFP cells, a promoter is separated from a GFP coding cassette by a puro gene that is flanked by two I-SceI sites in the same orientation. Once the puro gene is excised by NHEJ repair of the two I-SceI-induced DSBs, the promoter is joined to the rest of the expression cassette, leading to restoration of the GFP+ gene.
We demonstrated that IR induced the expression of Cav-1 (Fig. 1), a phenomenon previously reported by others , , , (Fig. 1), but we also found that the increased expression of Cav-1 protein by IR does not appear to result from activation of Cav-1 transcription, as the mRNA level of Cav-1 was not affected by the treatments (Fig. 2). The exact mechanism in which Cav-1 increased after DNA damage remains to be elucidated. Our observation on the roles of Cav-1 in activating DNA repair signaling (Fig. 3, 4, and 5) may explain the pro-survival function of Cav-1 in IR-treated cells, as shown by us (Fig. 10) and others , , . Notably, we found that Cav-1 could be up-regulated within 30 min following IR treatment (Fig. 1), earlier than the 24 h shown by Cordes et al , suggesting that Cav-1 may act as a sensor and early mediator in response to DNA damage.
In this study we have begun to elucidate the mechanisms by which Cav-1 regulates DNA repair. We demonstrated that Cav-1 participates in both HR and NHEJ repair pathways. The effect of Cav-1 on HR was demonstrated by the experiments showing that silencing of Cav-1 expression decreased HR frequency (Fig. 8). The role of Cav-1 in HR might be related to, at least in part, its effect on the accumulation of BRCA1 foci in nuclei after DNA damage (Fig. 5), which was verified by cell cycle analysis showing that knockdown of Cav-1 did not alter cell cycle distribution, a factor known to affect the foci formation of BRCA1 protein . Reciprocal regulation of the expression of Cav-1 and BRCA1 has been reported , , but whether this is associated with the Cav-1-mediated BRCA1 nuclear accumulation remains to be clarified. The role of Cav-1 in NHEJ was supported by our observation that suppression of Cav-1 by siRNA dramatically inhibited the IR-activated phosphorylation (Ser2056) of DNA-PK (Fig. 9A), one of the key executers in the NHEJ system, and by the GFP-based chromosomal reporter assay showing that the frequency of NHEJ was significantly higher in HEK293 cells transfected with a Cav-1 expression vector than in the cells transfected with a control vector (Fig. 9B). The mechanism of these effects might involve the Cav-1-mediated nuclear translocation of EGFR, an activator of DNA-PK , as Cav-1-targeted siRNA also inhibited the co-translocation of Cav-1 and EGFR following IR treatment (Fig. 9C and D). Therefore, it is likely that the signaling – modulating molecule, Cav-1, may facilitate DNA repair via multiple pathways. How precisely Cav-1 regulates HR and NHEJ and whether Cav-1 is involved in other DNA repair pathways remain to be studied.
Our results may provide a possible explanation for the differential expression of Cav-1 at various stages of tumor progression. As genome instability triggered by endogenous or exogenous DNA damaging agents is one of the main causes of cancer, loss or deficiency of Cav-1 at early stages of cancer development may cause a defect in DNA damage response leading to genomic alteration and oncogenic transformation. However, re-expression of Cav-1 at later stages of cancer may provide a protective mechanism for cancer cells to survive various harsh conditions such as DNA damage. In fact, the protective effects of Cav-1 against mechanical shearing damage, hypoxia, and nutrient depletion, the stresses that are considered the causes for death of tumor cells during their migration and metastasis, have been reported recently , , , , . Thus, re-expression of Cav-1 at advanced stages of cancer may provide a survival mechanism for tumor cells, and targeting Cav-1 may represent a new stratagem for cancer treatment.
Taken together, our study reveals a novel function for Cav-1 in repairing DNA, which involves both HR and NHEJ, and suggests that Cav-1 may play a critical role in orchestrating the response of cells to DNA damage and in mediating DNA repair.
Materials and Methods
MDA-MB-468 (human breast cancer cell), MCF-7 (human breast cancer cell), MCF-10A (human mammary epithelial cell), PC-3 (human prostate cancer cell) and T98G (human glioma cell) lines were purchased from American Type Culture Collection (Rockville, MD). NCI/ADR-RES line (ovarian cancer cell line) (previously named MCF-7/AdrR) was provided by Dr. Kenneth Cowan of the Eppley Institute for Research in Cancer (Omaha, NE). HT1080 (human fibrosarcoma cell) line was obtained from Dr. Mark Brenneman (Rutgers University, Piscataway, NJ). MCF-7, PC-3 and NCI/ADR-RES cell lines were maintained in RPMI 1640 medium (Invitrogen Life Technologies, Gaithersburg, MD); MDA-MB-468 and HT1080 cell lines in Dulbecco's modified Eagle's medium (Invitrogen Life Technologies); T98G in Ham's F-10/DMEM (10:1) medium (Invitrogen Life Technologies); and MCF-10A in DMEM/F12 (Invitrogen Life Technologies) supplemented with 5% donor horse serum, 20 ng/ml epidermal growth factor, 10 µg/ml insulin, 0.5 µg/ml hydrocortisone and 100 ng/ml cholera toxin (Sigma, St. Louis, MO). All the culture media contained 100 units/ml penicillin and 100 µg/ml streptomycin (Invitrogen Life Technologies, Gaithersburg, MD); all the cell lines were cultured and grown in a 5% CO2 - humidified incubator at 37°C.
Cells in exponential phase of growth were plated in 60-mm cell culture plates at 1×106 cells/plate and incubated for overnight, and then transfected with 100 nM of Cav-1 siRNA or a non-target RNA (Dharmacon, Inc, Lafayette, CO) using Lipofectamine 2000 and OPTI-MEM I reduced serum medium (Invitrogen Life Technologies, Gaithersburg, MD), according to the manufacturer's protocol. Silencing effects of siRNA were examined by Western blot and real-time RT-PCR.
Western blot analysis
Cells were washed twice with PBS containing a Protease Inhibitor Cocktail (Pierce Biotechnology Inc., Rockford, IL) and lysed with CelLytic™ MT Cell Lysis Reagent (Sigma-Aldrich, St. Louis, MO). Lysates were transferred to 1.5-ml eppendorf tubes and clarified by centrifugation at 16,000×g for 25 min at 4°C. Equal amounts of cell lysates (25 µg proteins) were resolved by SDS-PAGE, and then transferred to nitrocellulose. The membranes were incubated in 5% nonfat milk in TBST (Tris-buffered saline plus 0.1% Tween 20) at room temperature for 1 h, followed by immunoblotting with the respective antibodies. Detection of proteins by enzymed-linked chemiluminescence was performed according to the manufacturer's protocol (ECL; Pierce Biotechnology Inc., Rockford, IL). Quantification of protein bands was performed using the ImageJ software (http://rsb.info.nih.gov/ij). The antibodies used and dilution ratio were: mouse anti-β-actin (AC-74), anti-tubulin (DM1A) antibodies (1:5000; Sigma-Aldrich, St. Louis, MO); mouse anti-BRCA1(AB-1) antibody (1:500; Calbiochem, La Jolla, CA); mouse anti-Cav-1 (Z034) (1:2000; Zymed Laboratories, San Francisco, CA, USA); rabbit anti-EGFR (1:1000; Cat. No. SC-03, Santa Cruz Biotech, Santa Cruz, CA); rabbit anti-H2AX (ab2893), anti-DNA PKcs (ab32566) and anti-DNA PKcs (phospho S2056) (ab18192) antibodies (1:2000, 1:1000 and 1:500; Abcam, Cambridge, UK); mouse anti-H2AX (phospho S139) (JBW301) antibody (1:2000; Upstate, Chicago, IL); mouse anti-PP2A-C (1D6) antibody (1:1000; Chemicon International, Chandlers Ford, UK); rabbit anti-ATM (D2E2), anti-ATM (phospho S1981) (10H11.E12)and anti-CHK2 (phospho T68) (C13C1) (1:2000, 1:1000 and 1:500; Cell Signaling Technology, Beverly, MA).
Quantitative real-time RT-PCR
Total RNAs from cells were extracted with TriZol Reagent (Invitrogen Life Technologies, Gaithersburg, MD) following the manufacturer's instruction. First strand cDNA synthesis and amplification were performed using Omniscript RT Kit (QIAGEN Valencia, CA). The following human CAV1 primers were used: forward: 5′-CAC ATC TGG GCA GTT GTA CC-3′; reverse: 5′-CAC AGA CGG TGT GGA CGT AG-3′ . The β-actin primers, designed by our laboratory , were as follows: forward: 5′-GCC AAC ACA GTG CTG TCT GG-3′; reverse 5′-GCT CAG GAG GAG CAA TGA TCT TG-3′. SYBR Green quantitative PCR amplifications were performed on the Stratagene 3005P Real-TimePCR system. Reactions were carried out in a 25-µl volume containing 12.5 µl of 2 SYBR Green PCR Master Mix (Bio-Rad). The thermal profile for the real-time PCR was 95°C for 3 min followed by 40 cycles of 95°C for 20 s, 59°C for 30 s, and 70°C for 30 s. The ΔCt data were collected automatically. The average ΔCt of each group was calculated by the following formula: ΔCt = average CAV1 gene Ct-average of HK (housekeeping) gene' Ct. ΔΔCt was calculated by ΔΔCt = ΔCt of non-target control group - ΔCt of the siRNA transfection group. The fold-change for CAV1 expression level was calculated using 2−ΔΔCt.
Cells were cultured on glass slides and stained as described previously . Briefly, cells were treated with 5 Gy of IR, and then fixed in PBS containing 4% paraformaldehyde (EMD Chemicals, Merck Corporation, San Diego, CA) at room temperature for 20 min. Fixed cells were rinsed with PBS and with 25 mM NH4Cl in PBS for 10 min to quench free aldehyde groups. The cells were permeabilized by incubation in freshly-prepared 0.1% Triton X-100/PBS for 15 min. The cells were pre-incubated for 1 h in PBS containing 3% bovine serum albumin (BSA) and incubated for 2 h in diluted antibodies in PBS containing 3% BSA. Following washing three times, the cells were incubated for 1 h in diluted flourescence–labeled secondary antibodies. After washing with PBS, immuno-stained cells were examined with a Zeiss LSM 510 Meta laser scanning confocal microscope or ApoTome Microscope (Carl Zeiss Ltd, Germany). Primay antibodies and dilution ratio were: rabbit anti-Cav-1 antibody (1:1000; ab2910, Abcam, Cambridge, UK); mouse anti-BRCA1 antibody (1:50; Calbiochem, La Jolla, CA); sheep anti-EGFR (1E4) antibody (1:400; Upstate, Chicago, IL); mouse anti-PP2A-C antibody (1:100; Chemicon International, Chandlers Ford, UK); mouse anti-H2AX (phospho S139) antibody (1:2000; Upstate, Chicago, IL). All secondary antibodies were purchased from Molecular Probes (Eugene, OR) and used at a dilution of 1:500.
Cells were washed with PBS, collected, and lysed with RIPA buffer (150 mM NaCl, 1% NP-40, 0.5% deoxycholate, 0.1% SDS, 50 mM Tris pH 8.0) containing Protease Inhibitor Cocktail (Pierce Biotechnology Inc., Rockford, IL). The lysates were sonicated and centrifuged at 16,000×g for 25 min at 4°C. The supernatant was pre-cleared with protein A/G agarose (1:25 dilution), and immunoprecipitation was carried out using the respective antibodies. The immuno-complexes were washed four times with RIPA buffer, and proteins were eluted with 2X SDS sample buffer by boiling for 5 min. Ten µl precipitated proteins were resolved on SDS–PAGE and subjected to Western blot analysis using the respective antibodies.
Immunofluorescent detection of ssDNA
Detection of ssDNA was carried out as reported . Briefly, cells were grown on cover slips for overnight, and then incubated in medium containing 30 mmol/l BrdU (Bromodeoxyuridien, Sigma) for 24 h in the dark. To visualize ssDNA, the cells were fixed with methanol at −20°C for 10 min and then incubated in blocking solution (2% bovine serum albumin in PBS) at room temperature for 30 min, followed by incubation with an anti-BrdU antibody (Becton Dickinson, Franklin Lakes, NJ, USA). The cells were washed four times with PBS and then incubated with rhodamine red-X- conjugated goat anti-mouse IgG (Jackson ImmunoResearch Laboratories, Inc.) for 30 min at room temperature in the dark. The cells were counterstained with DAPI in blue for total DNA. Fluorescent images were taken using Carl Zeiss fluorescent microscope (Axiovert-200M) equipped with a Carl Zeiss digital camera (AxioCam MRC). The nuclear areas were selected using the ImageJ v1.37 software (http://rsb.info.nih.gov/ij/) and fluorescent signals from ssDNA and total DNA were integrated. The ratio of ssDNA signal intensity to total DNA represents the relative level of ssDNA in the nucleus. For each experiment, at least 30 cells were analyzed. Data were reported as mean ± SE from five independent experiments. Statistical significance of fluorescent signal intensity and ratio of signal intensity in cells with or without silencing of Cav-1 were analyzed by two-tailed t-test.
Human HT1080 cells were transfected with either a Cav-1 siRNA or a non-targeting RNA. Two days after transfection, cells were trypsinized and resuspended in gene pulser electroporation buffer. Four µg of an I-SceI expression vector pCMV(3_NLS) HA-I-SceI or an empty vector were introduced into 3.5×105 cells by electroporation. The cells were then seeded at 85,000 cells/100-mm culture dish for puromycin selection. The seeded cell cultures were re-fed with fresh medium containing 1 µg/ml puromycin on day 2 following electroporation, and the puromycin - containing medium was changed on days 6, 10, 12, and 14 days. At the end of selection, cells were fixed and stained, and colonies with 50 or more cells were counted.
NHEJ frequency assay
The frequency of total NHEJ was determined using a GFP-based chromosomal reporter, EJ5-GFP, as previously described by Bennardo et al. . Briefly, the transformed human embryonic kidney HEK293 cells containing a GFP-based chromosomal reporter, EJ5-GFP, were transfected with a caveolin-1 expression vector or a control empty vector. Thirty-six hours later, the cells were transfected with an HA tagged I-SceI endonuclease expression vector or a control empty vector. Seventy-two hours following transfection with the HA-I-I-SceI plasmid, percentage of EGFP expressing cells, which represents the frequency of NHEJ, were determined by flow cytometry.
Analysis of cell cycle distribution
Cells were trypsinized, washed, and fixed with 80% ethanol for 1 hour. Following treatment of cells with RNase and propidium iodide (Sigma, St. Louis, MO), cell cycle distribution (5,000 cells) was analyzed by fluorescence activated cell sorting (FACS) using a flow cytometer (Coulter Cytomics FC, Beckman Coulter, Miami, FL).
Colony formation assay
The numbers of cells to be plated for each IR dose and drug concentration were determined by a pilot experiment in order to yield 50–150 surviving colonies/100-mm plate. For IR tests, cells were plated and incubated for 18 h at 37°C, and then were irradiated with a Cs-137 γ-irradiator (Nordion Inc., Canada). Two weeks after IR treatment, colonies were fixed with methanol and stained with 1% crystal violet. To calculate the survival fraction, number of colonies was normalized to the number of cells plated. For drug tests, cells in 60 - mm plates were treated with bleomycin (EMD Chemicals, Merck Corporation, San Diego, CA) for 2 h, and then the drug was washed off with drug-free medium. The survival fractions were calculated as described above.
Student's t-test was used to determine the degree of significance.
We are grateful to Dr. Jeremy Stark for providing us with the EJ5-GFP expressing HEK293 cells and other reagents for NHEJ assay. We thank Jeremy Haakenson for helpful discussion of this work.
Conceived and designed the experiments: HZ ZS JMY. Performed the experiments: HZ JY ZP HW YC MY. Analyzed the data: HZ JY ZP HW YC HL XR ZS JMY. Wrote the paper: HZ HL XR JMY.
- 1. Bouras T, Lisanti MP, Pestell RG (2004) Caveolin-1 in breast cancer. Cancer Biol Ther 3: 931–941.
- 2. Burgermeister E, Liscovitch M, Rocken C, Schmid RM, Ebert MP (2008) Caveats of caveolin-1 in cancer progression. Cancer Lett 268: 187–201.
- 3. Burgermeister E, Xing X, Rocken C, Juhasz M, Chen J, et al. (2007) Differential expression and function of caveolin-1 in human gastric cancer progression. Cancer Res 67: 8519–8526.
- 4. Carver LA, Schnitzer JE (2003) Caveolae: mining little caves for new cancer targets. Nat Rev Cancer 3: 571–581.
- 5. Engelman JA, Zhang XL, Lisanti MP (1998) Genes encoding human caveolin-1 and -2 are co-localized to the D7S522 locus (7q31.1), a known fragile site (FRA7G) that is frequently deleted in human cancers. FEBS Lett 436: 403–410.
- 6. Sagara Y, Mimori K, Yoshinaga K, Tanaka F, Nishida K, et al. (2004) Clinical significance of Caveolin-1, Caveolin-2 and HER2/neu mRNA expression in human breast cancer. Br J Cancer 91: 959–965.
- 7. Bender FC, Reymond MA, Bron C, Quest AF (2000) Caveolin-1 levels are down-regulated in human colon tumors, and ectopic expression of caveolin-1 in colon carcinoma cell lines reduces cell tumorigenicity. Cancer Res 60: 5870–5878.
- 8. Kato T, Miyamoto M, Kato K, Cho Y, Itoh T, et al. (2004) Difference of caveolin-1 expression pattern in human lung neoplastic tissue. Atypical adenomatous hyperplasia, adenocarcinoma and squamous cell carcinoma. Cancer Lett 214: 121–128.
- 9. Racine C, Belanger M, Hirabayashi H, Boucher M, Chakir J, et al. (1999) Reduction of caveolin 1 gene expression in lung carcinoma cell lines. Biochem Biophys Res Commun 255: 580–586.
- 10. Sunaga N, Miyajima K, Suzuki M, Sato M, White MA, et al. (2004) Different roles for caveolin-1 in the development of non-small cell lung cancer versus small cell lung cancer. Cancer Res 64: 4277–4285.
- 11. Bagnoli M, Tomassetti A, Figini M, Flati S, Dolo V, et al. (2000) Downmodulation of caveolin-1 expression in human ovarian carcinoma is directly related to alpha-folate receptor overexpression. Oncogene 19: 4754–4763.
- 12. Wiechen K, Diatchenko L, Agoulnik A, Scharff KM, Schober H, et al. (2001) Caveolin-1 is down-regulated in human ovarian carcinoma and acts as a candidate tumor suppressor gene. Am J Pathol 159: 1635–1643.
- 13. Wiechen K, Sers C, Agoulnik A, Arlt K, Dietel M, et al. (2001) Down-regulation of caveolin-1, a candidate tumor suppressor gene, in sarcomas. Am J Pathol 158: 833–839.
- 14. Aldred MA, Ginn-Pease ME, Morrison CD, Popkie AP, Gimm O, et al. (2003) Caveolin-1 and caveolin-2,together with three bone morphogenetic protein-related genes, may encode novel tumor suppressors down-regulated in sporadic follicular thyroid carcinogenesis. Cancer Res 63: 2864–2871.
- 15. Lee SW, Reimer CL, Oh P, Campbell DB, Schnitzer JE (1998) Tumor cell growth inhibition by caveolin re-expression in human breast cancer cells. Oncogene 16: 1391–1397.
- 16. Wu P, Wang X, Li F, Qi B, Zhu H, et al. (2008) Growth suppression of MCF-7 cancer cell-derived xenografts in nude mice by caveolin-1. Biochem Biophys Res Commun 376: 215–220.
- 17. Hayashi K, Matsuda S, Machida K, Yamamoto T, Fukuda Y, et al. (2001) Invasion activating caveolin-1 mutation in human scirrhous breast cancers. Cancer Res 61: 2361–2364.
- 18. Williams TM, Cheung MW, Park DS, Razani B, Cohen AW, et al. (2003) Loss of caveolin-1 gene expression accelerates the development of dysplastic mammary lesions in tumor-prone transgenic mice. Mol Biol Cell 14: 1027–1042.
- 19. Rajjayabun PH, Garg S, Durkan GC, Charlton R, Robinson MC, et al. (2001) Caveolin-1 expression is associated with high-grade bladder cancer. Urology 58: 811–814.
- 20. Elsheikh SE, Green AR, Rakha EA, Samaka RM, Ammar AA, et al. (2008) Caveolin 1 and Caveolin 2 are associated with breast cancer basal-like and triple-negative immunophenotype. Br J Cancer 99: 327–334.
- 21. Pinilla SM, Honrado E, Hardisson D, Benitez J, Palacios J (2006) Caveolin-1 expression is associated with a basal-like phenotype in sporadic and hereditary breast cancer. Breast Cancer Res Treat 99: 85–90.
- 22. Savage K, Lambros MB, Robertson D, Jones RL, Jones C, et al. (2007) Caveolin 1 is overexpressed and amplified in a subset of basal-like and metaplastic breast carcinomas: a morphologic, ultrastructural, immunohistochemical, and in situ hybridization analysis. Clin Cancer Res 13: 90–101.
- 23. Patlolla JM, Swamy MV, Raju J, Rao CV (2004) Overexpression of caveolin-1 in experimental colon adenocarcinomas and human colon cancer cell lines. Oncol Rep 11: 957–963.
- 24. Ando T, Ishiguro H, Kimura M, Mitsui A, Mori Y, et al. (2007) The overexpression of caveolin-1 and caveolin-2 correlates with a poor prognosis and tumor progression in esophageal squamous cell carcinoma. Oncol Rep 18: 601–609.
- 25. Kato K, Hida Y, Miyamoto M, Hashida H, Shinohara T, et al. (2002) Overexpression of caveolin-1 in esophageal squamous cell carcinoma correlates with lymph node metastasis and pathologic stage. Cancer 94: 929–933.
- 26. Ho CC, Kuo SH, Huang PH, Huang HY, Yang CH, et al. (2008) Caveolin-1 expression is significantly associated with drug resistance and poor prognosis in advanced non-small cell lung cancer patients treated with gemcitabine-based chemotherapy. Lung Cancer 59: 105–110.
- 27. Tanase CP (2008) Caveolin-1: a marker for pancreatic cancer diagnosis. Expert Rev Mol Diagn 8: 395–404.
- 28. Satoh T, Yang G, Egawa S, Addai J, Frolov A, et al. (2003) Caveolin-1 expression is a predictor of recurrence-free survival in pT2N0 prostate carcinoma diagnosed in Japanese patients. Cancer 97: 1225–1233.
- 29. Campbell L, Gumbleton M, Griffiths DF (2003) Caveolin-1 overexpression predicts poor disease-free survival of patients with clinically confined renal cell carcinoma. Br J Cancer 89: 1909–1913.
- 30. Joo HJ, Oh DK, Kim YS, Lee KB, Kim SJ (2004) Increased expression of caveolin-1 and microvessel density correlates with metastasis and poor prognosis in clear cell renal cell carcinoma. BJU Int 93: 291–296.
- 31. Lavie Y, Fiucci G, Liscovitch M (2001) Upregulation of caveolin in multidrug resistant cancer cells: functional implications. Adv Drug Deliv Rev 49: 317–323.
- 32. Shatz M, Liscovitch M (2004) Caveolin-1 and cancer multidrug resistance: coordinate regulation of pro-survival proteins? Leuk Res 28: 907–908.
- 33. Cordes N, Frick S, Brunner TB, Pilarsky C, Grutzmann R, et al. (2007) Human pancreatic tumor cells are sensitized to ionizing radiation by knockdown of caveolin-1. Oncogene 26: 6851–6862.
- 34. Hehlgans S, Eke I, Storch K, Haase M, Baretton GB, et al. (2009) Caveolin-1 mediated radioresistance of 3D grown pancreatic cancer cells. Radiother Oncol.
- 35. Lio YC, Schild D, Brenneman MA, Redpath JL, Chen DJ (2004) Human Rad51C deficiency destabilizes XRCC3, impairs recombination, and radiosensitizes S/G2-phase cells. J Biol Chem 279: 42313–42320.
- 36. Lobrich M, Jeggo PA (2007) The impact of a negligent G2/M checkpoint on genomic instability and cancer induction. Nat Rev Cancer 7: 861–869.
- 37. Bennardo N, Cheng A, Huang N, Stark JM (2008) Alternative-NHEJ is a mechanistically distinct pathway of mammalian chromosome break repair. PLoS Genet 4: e1000110.
- 38. Chen DJ, Nirodi CS (2007) The epidermal growth factor receptor: a role in repair of radiation-induced DNA damage. Clin Cancer Res 13: 6555–6560.
- 39. Del Pozo MA, Schwartz MA (2007) Rac, membrane heterogeneity, caveolin and regulation of growth by integrins. Trends Cell Biol 17: 246–250.
- 40. Ravid D, Maor S, Werner H, Liscovitch M (2005) Caveolin-1 inhibits cell detachment-induced p53 activation and anoikis by upregulation of insulin-like growth factor-I receptors and signaling. Oncogene 24: 1338–1347.
- 41. Glait C, Tencer L, Ravid D, Sarfstein R, Liscovitch M, et al. (2006) Caveolin-1 up-regulates IGF-I receptor gene transcription in breast cancer cells via Sp1- and p53-dependent pathways. Exp Cell Res 312: 3899–3908.
- 42. Zhu H, Weisleder N, Wu P, Cai C, Chen JW (2008) Caveolae/caveolin-1 are important modulators of store-operated calcium entry in Hs578/T breast cancer cells. J Pharmacol Sci 106: 287–294.
- 43. Dittmann K, Mayer C, Kehlbach R, Rodemann HP (2008) Radiation-induced caveolin-1 associated EGFR internalization is linked with nuclear EGFR transport and activation of DNA-PK. Mol Cancer 7: 69.
- 44. Ahn M, Kim H, Kim JT, Lee J, Hyun JW, et al. (2006) Gamma-ray irradiation stimulates the expression of caveolin-1 and GFAP in rat spinal cord: a study of immunoblot and immunohistochemistry. J Vet Sci 7: 309–314.
- 45. Scully R, Chen J, Ochs RL, Keegan K, Hoekstra M, et al. (1997) Dynamic changes of BRCA1 subnuclear location and phosphorylation state are initiated by DNA damage. Cell 90: 425–435.
- 46. Wang Y, Yu J, Zhan Q (2008) BRCA1 regulates caveolin-1 expression and inhibits cell invasiveness. Biochem Biophys Res Commun 370: 201–206.
- 47. Glait C, Ravid D, Lee SW, Liscovitch M, Werner H (2006) Caveolin-1 controls BRCA1 gene expression and cellular localization in human breast cancer cells. FEBS Lett 580: 5268–5274.
- 48. Milovanova T, Chatterjee S, Hawkins BJ, Hong N, Sorokina EM, et al. (2008) Caveolae are an essential component of the pathway for endothelial cell signaling associated with abrupt reduction of shear stress. Biochim Biophys Acta 1783: 1866–1875.
- 49. Ravid D, Maor S, Werner H, Liscovitch M (2006) Caveolin-1 inhibits anoikis and promotes survival signaling in cancer cells. Adv Enzyme Regul 46: 163–175.
- 50. Patel HH, Tsutsumi YM, Head BP, Niesman IR, Jennings M, et al. (2007) Mechanisms of cardiac protection from ischemia/reperfusion injury: a role for caveolae and caveolin-1. FASEB J 21: 1565–1574.
- 51. Dasari A, Bartholomew JN, Volonte D, Galbiati F (2006) Oxidative stress induces premature senescence by stimulating caveolin-1 gene transcription through p38 mitogen-activated protein kinase/Sp1-mediated activation of two GC-rich promoter elements. Cancer Res 66: 10805–10814.
- 52. Frank PG, Lisanti MP (2006) Role of caveolin-1 in the regulation of the vascular shear stress response. J Clin Invest 116: 1222–1225.
- 53. Li T, Sotgia F, Vuolo MA, Li M, Yang WC, et al. (2006) Caveolin-1 mutations in human breast cancer: functional association with estrogen receptor alpha-positive status. Am J Pathol 168: 1998–2013.
- 54. Zhu H, Wu H, Liu X, Evans BR, Medina DJ, et al. (2008) Role of MicroRNA miR-27a and miR-451 in the regulation of MDR1/P-glycoprotein expression in human cancer cells. Biochem Pharmacol 76: 582–588.
- 55. Zhu H, Cai C, Chen J (2004) Suppression of P-glycoprotein gene expression in Hs578T/Dox by the overexpression of caveolin-1. FEBS Lett 576: 369–374.
- 56. Lu H, Yue J, Meng X, Nickoloff JA, Shen Z (2007) BCCIP regulates homologous recombination by distinct domains and suppresses spontaneous DNA damage. Nucleic Acids Res 35: 7160–7170.