Perturbation of DNA repair pathways by proteasome inhibitors corresponds to enhanced chemosensitivity of cells to DNA damage-inducing agents
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- Takeshita, T., Wu, W., Koike, A. et al. Cancer Chemother Pharmacol (2009) 64: 1039. doi:10.1007/s00280-009-0961-5
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Breast cancer treatment often employs DNA double-strand breaks (DSBs), such as that induced by irradiation or anticancer agents. Ubiquitination is required at the site of DNA damage and plays a crucial role in the DSB repair pathway. We investigated the effect of proteasome inhibitors on the pathway after exposure to chemotherapeutic agents and examined its correlation with cytotoxicity.
Cells were exposed for 1 h to DNA damage-inducing chemotherapeutic agents. After DNA damage, nuclear foci formation of conjugated ubiquitin (Ub-foci) and cell viability were examined in the absence or presence of proteasome inhibitors MG132 and epoxomicin.
Proteasome inhibitors trapped conjugated ubiquitin in the cytosol and blocked irinotecan (CPT-11)- and epirubicin-induced Ub-foci formation in MCF10A cells and HeLa cells, but not in MCF7 cells. MG132 sensitized MCF10A cells to CPT-11 and epirubicin treatment, demonstrating a synergistic effect. This synergistic effect is likely due to the failure to repair DNA, because a significant rise in unrepaired DNA damage was observed in the cells treated with MG132. On the other hand, no synergy was observed in MCF7 cells or when MG132 was combined with docetaxel.
The synergistic effect of proteasome inhibitors in combination with DNA damage-inducing agents warrants further investigating into its effectiveness in the treatment of breast cancer.
KeywordsChemosensitivityUbiquitinProteasome inhibitorNuclear foci formationDNA damage
Induction of DNA double-strand breaks (DSBs) by irradiation or anticancer agents is a major strategy employed for breast cancer treatment. DSBs cause breast cancer cells to undergo apoptosis when appropriate repair pathways, such as those mediated by BRCA1, are perturbed. Therefore, chemosensitivity and the competence of DNA damage repair pathways are closely correlated. For example, it was recently reported that acquired resistance to cisplatin or PARP inhibitor in BRCA1- or BRCA2-mutated tumors can be mediated by secondary mutations in these genes that restore the wild-type reading frame [1–3].
Recently, the cascade of events in response to DSBs has been significantly uncovered. The sequential recruitment of repair proteins at the site of DNA damage includes two RING finger type E3 ubiquitin ligases, RNF8 and BRCA1. RNF8 catalyzes lysine 63-linked polyubiquitin (K63-Ub) chains on H2AX [4–7]. Ubiquitinated H2AX then recruits the BRCA1/Abraxas/RAP80 complex through the RAP80 subunit, an adaptor that contains UIM (ubiquitin interacting motif) domains [8–10]. BRCA1 forms a RING heterodimer E3 ubiquitin ligase with BARD1  and is required for the recruitment of BRCA2 and Rad51 to damaged sites for homologous recombination repair . Thus, ubiquitination is involved in key steps that properly conduct the homologous recombination repair pathway after DSBs. Indeed, inhibition of IR-induced nuclear foci (IRIF) formation of conjugated ubiquitin results in defective downstream events, including BRCA1 IRIF formation and IR hypersensitivity [5–7, 13].
Ubiquitin modification regulates a wide range of cellular pathways such as removal of misfolded or aged housekeeping proteins, protein trafficking, the cellular immune response by antigenic peptide processing, the cell cycle and the DNA damage response. Ubiquitin modification requires several critical enzymes: a ubiquitin-activating enzyme (E1), a ubiquitin carrier protein (E2), and a ubiquitin ligase (E3) . The E3 catalyzes the formation of polyubiquitin chains (and sometimes monoubiquitination), utilizing ubiquitins that have been activated by the E1 and E2 enzymes, and transfers them onto specific substrate(s). While ubiquitin modifications signal a variety of processes depending upon the type of ubiquitin chains, the most common pathway is the ubiquitin-proteasome system (UPS) that is mediated by Lys48-linked polyubiquitin chains [14, 15]. Substrates conjugated with Lys48-linked chains are recognized by the 19S regulatory cap subunits of the 26S proteasome and are degraded by the 20S catalytic core subunits . These reactions can be inhibited by proteasome inhibitors such as MG132, epoxomicin or the clinically used bortezomib (PS-341, Velcade®).
The effect of proteasome inhibitors on the response to DNA damage is not fully understood. Because the known major ubiquitin chains built at the damaged site in response to DSBs are Lys63- and Lys6-linked [9, 15, 17], the direct effect of the proteasome inhibitor could be limited. Interestingly, recent studies showed that inhibition of the 26S proteasome by MG132 depleted the pool of available nuclear ubiquitin because undegraded polyubiquitinated proteins accumulated in the cytosol [5, 18]. The depletion of free nuclear ubiquitin resulted in the loss of IRIF formation of conjugated ubiquitin, accompanied by loss of BRCA1- and 53BP1-IRIF formations . This suggests the possibility that proteasome inhibitors may also inhibit the repair pathway of DNA damage caused by treatment with DNA damage-inducing chemotherapeutic agents, thereby having an additive or synergistic effect on cytotoxicity. In this regard, we investigated the effect of proteasome inhibitors on the cellular distribution of conjugated ubiquitin and its correlation with chemotherapeutic agent-induced nuclear foci formation and cytotoxicity. The results suggest that the effect of the proteasome inhibitors on ubiquitin distribution varies among cell lines and that it correlates with the DNA damage response and chemosensitivity.
Materials and methods
MCF7 breast carcinoma cells and HeLa cervical carcinoma cells were cultured in Dulbecco’s Modified Eagle’s Medium (DMEM) supplemented with 10% fetal calf serum (FCS) and 1% antibiotic–antimycotic agent (Life Technologies, Inc, Grand Island, NY) in 5% CO2 at 37°C. MCF10A normal human breast epithelial cells were grown in DMEM/Ham’s F12 (1:1) medium supplemented with 2.5% FCS, 100 ng/ml cholera toxin, 20 ng/ml epidermal growth factor, 500 ng/ml hydrocortisone, 10 mg/ml insulin and 1% antibiotic–antimycotic agent. Cells were seeded at a concentration of 1.5 × 103 cells per well in flat-bottom 96-well microplates or 5.0 × 104 cells per well in Lab-Tek eight-well chamber slides (Nalge Nunc) for the study of cell viability or immunofluorescence, respectively, 24 h before treatment with proteasome inhibitor and/or chemotherapeutic agents. For induction of DNA damage with chemotherapeutic agents, cells were incubated for 1 h with the indicated doses of either CPT-11 (Sigma, Saint Louis, MO) or epirubicin (Pfizer, New York, NY). Cells were washed with phosphate buffered saline (PBS) and further incubated in the culture medium with or without proteasome inhibitors. In some experiments, docetaxel (TAXOLTM, Sanofi-aventis K.K. Tokyo, Japan) was added instead of the DNA-damaging agents. Proteasome inhibitors MG132 (Calbiochem, San Diego, CA) or epoxomicin (Millennium Pharma, Cambridge, MA) or solvent DMSO was added at the indicated doses simultaneously with the chemotherapeutic agents and was maintained after the removal of the chemotherapeutic agents.
Indirect immunocytochemistry was performed as previously described with one modification . Briefly, proliferating cells were fixed with 3% formalin for 15 min and permeabilized with 0.2% Triton X-100 for 5 min. Cells were washed with PBS, blocked with 0.5% bovine serum albumin in PBS and incubated with a monoclonal antibody to conjugated ubiquitin (FK2, Nippon Bio-Test, Japan) diluted in the blocking buffer (10 μg/ml). FITC-conjugated anti-mouse IgG (Jackson Immuno Research, West Grove, PA) was used as the secondary antibody at a 1:25 dilution. For double staining with phosphorylated H2AX (γH2AX), a monoclonal antibody to γH2AX (upstate, Lake Placid, NY) was directly fluorescently labeled with Alexa Fluor® 555 (Invitrogen, Carlsbad, CA) according to the manufacturer’s instructions and was added to the cells previously stained with anti-conjugated ubiquitin. Cells were washed and re-fixed with 3% formalin for 15 min. After washing three times, the nucleus was counterstained with DAPI-containing fluorescent mounting medium (Invitrogen, Carlsbad, CA), and the cells were examined with a confocal laser scanning microscope (LSM 510, Carl Zeiss).
Measurements of chemosensitivity
Twenty-four hours after release from transient exposure to chemotherapeutic agents, cell viabilities were determined with the CellTiter 96® Aqueous One Solution Cell Proliferation Assay (Promega Corp., Madison, WI) according to the manufacturer’s instructions. Briefly, 6 μM CellTiter 96® Aqueous One Solution Reagent was directly added to the culture medium of cells in 96-well plates, incubated for 2 h, and the quantity of formazan product was measured by light absorbance at 570 nm primary wavelength and 600 nm reference wavelength by scanning with a 96-well plate reader (multi-spectrophotometer, DAINIPPON, Osaka, Japan). The percentages of cell viability are exhibited as the mean of triplicate experiments, where cells not exposed to chemotherapeutic agents or MG132 represent 100% viability.
Neutral comet assays were performed using the Trevigen’s CometAssay kit (4250-050-K) according to the manufacturer’s instructions. DNA was stained with Trevigen SYBR green, and Comet images were examined with a confocal laser scanning microscope (LSM 510, Carl Zeiss). Tail moments were analyzed by the TriTek CometScore Freeware program. The average value of tail moments was determined by counting at least 100 cells per sample.
Effect of proteasome inhibitors on the cellular distribution of conjugated ubiquitin
Proteasome inhibitors block CPT-11-induced Ub-foci formation at the site of DNA damage
The effect of proteasome inhibitors on Ub-foci formation varies among cell lines
A proteasome inhibitor modulates chemosensitivity of cells in correlation with its effect on Ub-foci formation
A proteasome inhibitor increases damaged DNA after treatment with CPT-11 or epirubicin
The UPS contributes to a wide range of cellular events and, therefore, the components of this pathway have become attractive, novel targets for therapeutic intervention. Breakthroughs have been achieved with the proteasome inhibitor bortezomib (Velcade, PS-341, Millennium) . Approximately a third of relapsed, refractory multiple myeloma patients showed a significant response to bortezomib , and the US FDA approved bortezomib for use as a therapy for multiple myeloma. Preclinical and early clinical studies suggested bortezomib is likely to be effective in solid tumors, and clinical trials in non-hematologic malignancies including breast cancer are ongoing. Phase II studies showed that bortezomib failed to show any objective response on metastatic advanced breast cancer when used as a single agent [26, 27]. However, the effect for selected patients, such as those with tumors expressing a particular hormone receptor, HER2 status or those in earlier stages of breast cancer, remain to be determined. In addition, recent clinical data have proven the efficacy of bortezomib in combination with several chemotherapeutic agents for breast cancer treatment [28–30].
The mechanisms underlying the therapeutic effect of bortezomib have been investigated intensively. In multiple myeloma, inhibition of the transcription factor NFκB by blocking the degradation of its inhibitory partner IκB is one such putative model . However, recent studies suggest that multiple factors might contribute to the efficacy of the drug. For DNA damage responses, depletion of ubiquitination at sites of DNA damage could be one of the major mechanisms leading cells to apoptosis. Proteasome inhibitors sensitize tumor cells to DNA damage-inducing chemotherapeutic agents [32, 33]. Particularly relevant for breast cancer, proteasome inhibitors sensitize myeloma cells to doxorubicin . One potent mechanism for this effect is that bortezomib down-regulates the expression of effectors involved in the cellular response to DNA damage . However, our result and a recent study reported from other laboratories [34, 35] suggest that there is an alternative mechanism where proteasome inhibitors perturb the ubiquitination-mediated DNA repair cascade. Proteasome inhibitors as well as depletion of 19S and 20S proteasome subunits inhibited DNA damage–signaling processes, including monoubiquitination and nuclear foci formation of FANCD2 and foci formation of phosphorylated ATM, 53BP1, NBS1, BRCA1 and RAD51 [34, 35]. The mechanisms responsible for inhibition remain unclear. Because PCNA monoubiquitination in response to DNA damage in cells treated with proteasome inhibitors was retained, it was speculated that free ubiquitin was still available to modify nuclear proteins at sites of DNA damage . However, it was recently reported that K63- or K6-linked polyubiquitination at DNA damaged sites is required for the recruitment of BRCA1 and 53BP1 [8–10] and that proteasome inhibitors inhibit nuclear foci formation of conjugated ubiquitin after IR . Our results show that proteasome inhibitors also inhibit foci formation after exposure to chemotherapeutic agents (Fig. 2, 3). Together, it is possible that proteasome inhibitors reduce the free ubiquitin pool in the nucleus to a level where monoubiquitination of PCNA is not affected but where polyubiquitination required for BRCA1/53BP1 recruitment is perturbed. The observation that FANCD2 foci formation was more severely affected than FANCD2 monoubiquitination in cells depleted for proteasome subunits  is consistent with this explanation.
Our results indicate that the effectiveness of proteasome inhibitors in terms of the cytosol trap of ubiquitin is remarkably different among cell lines. These differences influence the capacity of Ub-foci formation and chemosensitivity. It was previously reported that bortezomib has differential cellular and molecular effects in human breast cancer cells . However, no relationship was observed between the effect of bortezomib on cell viability and expression of HER-2, epidermal growth factor receptor, AKT or ERK1/2 . From our results, it is possible that the capacity of Ub-foci formation may cause the observed differential effects of bortezomib on cytotoxicity.
Recent studies in gene expression profiling identified specific subtypes of breast cancer with biologic and therapeutic implications. One particular subset, basal-like breast cancer expressing basal/myoepithelial cell markers such as cytokeratin 5/6, 14, 17 or Vimentin but not expressing estrogen receptor, progesterone receptor or HER2, exhibited an aggressive phenotype and a particularly poor prognosis [37–39]. Evidence from multiple sources strongly indicates that impairment of BRCA1 pathways is responsible for this phenotype [40–43]. Therefore, it is expected that this phenotype could be sensitive to DNA damage-inducing agents such as topoisomerase inhibitors, DNA cross-linkers or PARP inhibitors. Because proteasome inhibitors sensitize cells to DNA damage-inducing agents, they could affect the efficacy of these agents in the treatment of basal-like breast cancer. Alternatively, proteasome inhibitors may perturb the ubiquitin-mediated BRCA1 cascade in luminal type breast cancers, leading the DNA repair pathway to mimic that of basal-like breast cancer.
Treatment of cells with proteasome inhibitors trapped conjugated ubiquitin in the cytosol causing failure of Ub-foci formation and failure to repair DNA in response to DNA damage-inducing chemotherapeutic agents. The degree of this effect varied among cell lines. Cells that exhibited cytosol trapping of ubiquitin upon treatment with proteasome inhibitors were sensitized to DNA damage-inducing agents, exhibiting lower rates of cell viability. In contrast, cells not exhibiting the trapping effect were resistant to the synergy between proteasome inhibitors and DNA damage-inducing agents. Our results suggest that the synergistic effect of proteasome inhibitors in combination with DNA damage-inducing agents warrants further investigation into its effectiveness in the treatment of breast cancer.
This study was supported by grants from Japan Society for the Promotion of Science and the Japanese Ministry of Education, Culture, Sports, Science and Technology. We thank Mrs. Rie Ogawa for secretarial assistance.
Conflict of interest statement
The authors declare that they have no competing interests.
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