Smad3, a component of the transforming growth factor β signaling cascade, contributes to G1 arrest in breast cancer cells. Cyclin D1/cyclin-dependent kinase 4 (CDK4) promotes G1-S–phase transition, and CDK phosphorylation of Smad3 has been associated with inhibition of Smad3 activity. We hypothesized that overexpression of cyclin D1 exerts tumorigenic effects in breast cancer cells through CDK4-mediated phosphorylation and inhibition of Smad3 and release of G1 arrest. Real-time quantitative reverse transcription-PCR and immunoblotting were used to evaluate expression of study proteins in cyclin D1–overexpressing breast cancer cells. Smad3 transcriptional activity and cell cycle control were examined in cells transfected with wild-type (WT) Smad3 or Smad3 with single or multiple CDK phosphorylation site mutations (M) in the presence or absence of the CDK4 inhibitor or cotransfection with cdk4 small interfering RNA (siRNA). Transfection of the Smad3 5M construct resulted in decreased c-myc and higher p15INK4B expression. Compared with WT Smad3, overexpression of the Smad3 T8, T178, 4M, or 5M mutant constructs resulted in higher Smad3 transcriptional activity. Compared with cells transfected with WT Smad3, Smad3 transcriptional activity was higher in cells overexpressing Smad3 mutant constructs and treated with the CDK4 inhibitor or transfected with cdk4 siRNA. Cells transfected with Smad3 T8 or T178 and treated with the CDK4 inhibitor showed an increase in the G1 cell population. Inhibition of CDK-mediated Smad3 phosphorylation released cyclin D1–regulated blockade of Smad3 transcriptional activity and recovered cell cycle arrest in breast cancer cells. Targeted inhibition of CDK4 activity may have a role in the treatment of cyclin D–overexpressing breast cancers. Mol Cancer Res; 8(10); 1375–87. ©2010 AACR.

The transforming growth factor β (TGFβ) superfamily consists of a large group of secreted polypeptide growth factors that bind transmembrane serine-threonine kinase receptor complexes (1, 2). TGFβ/activin signaling is transduced through receptor-mediated phosphorylation of intracellular Smad2 and Smad3, which form a complex with Smad4, translocate to the nucleus, and, along with coactivators and cell-specific DNA-binding factors, regulate target gene expression relevant to several aspects of cell growth and differentiation (3-5). The significance of TGFβ signaling in breast cancer has been widely studied, although less is understood about the relevance of Smad-mediated transcriptional activity in cancer cell growth control (6).

Several lines of evidence suggest that Smad3 may be involved in cell cycle arrest. The Smad3 cofactors E2F4/5 and p107, along with Smad4, bind to a Smad-E2F site on c-myc, causing repression of this cell cycle mitogen (7). Furthermore, a nuclear Smad complex that includes Smad3 and the transcription factor Sp1 is thought to mediate transcription of the cyclin-dependent kinase (CDK) inhibitors p15 and p21, whose promoters contain an Sp1-binding site (8, 9). Additionally, Smad3/4 complexes, along with the forkhead box O protein, bind promoters responsible for transcription of p15 and p21 (10). Conversely, c-myc overexpression can inhibit the Smad-dependent transcription of p15 and p21 (11). Thus, working in conjunction with several different critical growth-regulatory mechanisms, Smad3 may act in a dual capacity to both inhibit c-myc expression and stimulate CDK inhibitor transcription to help actualize G1-phase cell cycle arrest. Consequently, the loss of Smad3 function could induce a potent cell cycle release, allowing for the uncontrolled cell growth characteristic of malignancy.

A relationship between Smad signaling and both normal and malignant mammary cell growth has been shown. Differential expression of activin and TGFβ receptors and Smads has been found in the mammary gland during pregnancy and lactation (12-14). In addition, in a breast cancer tissue microarray study, Xie et al. (15) showed that the loss of Smad4 correlated with axillary lymph node involvement, and the loss of phosphorylated Smad2 correlated with decreased overall survival. Subsequent work examining a panel of MCF-10A premalignant and transformed malignant mammary cell lines showed that Smad2/3 signaling conferred both tumor-suppressant and oncogenic effects, dependent on the primary or metastatic environment (16). Decreased levels of nuclear Smad3 have also been associated with larger tumor size, higher tumor grade, and estrogen receptor–negative breast cancers (17). These data point toward a dynamic role for Smad signaling in breast cancer, favoring a tumor-suppressant function in well-differentiated, earlier-stage disease.

The potential mechanisms responsible for circumvention of Smad-mediated cell growth control are being explored. Matsuura et al. have found Smad3 activity to be negatively regulated by CDK4 and CDK2 phosphorylation in fibroblasts (18, 19). Several Smad3-inhibitory CDK phosphorylation sites have been identified, primarily within the linker region of the molecule (5, 18). Cyclin D exerts its action via CDK4, and in Mv1Lu mink lung epithelial cells, cyclin D overexpression was found to induce Smad3 linker phosphorylation via CDK4, which led to inhibition of wild-type (WT) Smad3 activity (18, 19). The cyclin D–CDK4/6 complex is critical to cell cycle progression, as it induces phosphorylation inhibition of the Rb protein. Rb protein phosphorylation permits E2F-mediated transcription of genes responsible for cell cycle mitogenesis (20, 21). Thus, as cyclin D regulates one of the key initiating factors for cell cycle progression, the overexpression of this protein may render cells vulnerable to malignant transformation.

It follows that overexpression of cyclin D has been found in aggressive breast cancers, and this overexpression is associated with a poor prognosis. Cyclin D overexpression is pervasive in human breast cancers, including heritable breast cancers with BRCA2 mutations (22-24). It has been shown that Smad3 and BRCA2 can synergize to affect their tumor-suppressant functions (25). Potentially, the mutation of BRCA2 found in some tumors overexpressing cyclin D contributes to the inhibition of Smad3 cell cycle control in these cancers (25). Additionally, both the Ras and human epidermal growth factor receptor 2 (HER2) oncogenes have been linked to cyclin D1 promoter activation in breast cancer. This finding implies that the known pathologic repercussions of Ras and neu overexpression in certain breast cancers involve cyclin D1/CDK4 (23, 26). Furthermore, patients with highly proliferative cancers, such as cancers that overexpress cyclins, tend to initially respond well to chemotherapy, although many of these patients ultimately recur. These poor outcomes point to critical resistant flaws in cell cycle control inherent to cancers that overexpress cyclins. The current study examines the effect of cyclin D overexpression and CDK4 phosphorylation on Smad3 action in breast cancer cell lines. We hypothesize that the oncogenic effects of cyclin D1 overexpression in breast cancer are induced, in part, through CDK4-mediated phosphorylation inhibition of Smad3 and loss of cell cycle arrest.

Cell culture and antibodies

MCF7, Hs578T, and T47D cells were obtained from the American Type Culture Collection and maintained in DMEM-F12, DMEM, or RPMI 1640, respectively. Culture medium was supplemented with antibiotics, 10% fetal bovine serum, and 0.01 mg/mL bovine insulin (Hs578T cells only). The study cells stably expressing empty vector or cyclin D1 were maintained in the same fashion as the parental lines. Anti–cyclin D1, anti-CDK2, anti-CDK4, anti–glyceraldehyde-3-phosphate dehydrogenase (GAPDH), and anti–β-actin antibodies were obtained from Santa Cruz Biotechnology; anti-Smad3 and anti–phospho-Smad antibodies were purchased from Cell Signaling Technology.

Generation of stable cell lines

Human cyclin D1 cDNA was inserted into the cytomegalovirus-driven pcDNA-DEST40 expression vector (Invitrogen) containing a neomycin resistance gene to obtain the pEXPR-cyclin D1–expressing plasmid. To create the vector control and cyclin D1–overexpressing (CD1) cell lines, cells were stably transfected with empty vector (pcDNA-DEST40) or pEXPR-cyclin D1 plasmids. Two days after transfection, stable clones were selected in medium containing 500 mg/mL G418 (Invitrogen). The resistant clones were maintained in G418 for 21 days. Cyclin D1 overexpression was verified by immunoblot analysis as shown in Fig. 1A.

FIGURE 1.

Cyclin D expression and activity in MCF7 and T47D stably transfected cells. A, protein extracts from stably transfected MCF7 or T47D clones were separated (30 μg/lane) on SDS-PAGE and subjected to immunoblot analysis with the indicated antibodies. B, CDK4 kinase assay radiographs and densitometric quantification in MCF7 and T47D study cell lines. C, CDK2 kinase assay radiographs and densitometric quantification in MCF7 and T47D study cell lines.

FIGURE 1.

Cyclin D expression and activity in MCF7 and T47D stably transfected cells. A, protein extracts from stably transfected MCF7 or T47D clones were separated (30 μg/lane) on SDS-PAGE and subjected to immunoblot analysis with the indicated antibodies. B, CDK4 kinase assay radiographs and densitometric quantification in MCF7 and T47D study cell lines. C, CDK2 kinase assay radiographs and densitometric quantification in MCF7 and T47D study cell lines.

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Immunoblotting

Briefly, cells were scraped, pelleted, and rinsed with ice-cold HEPES-buffered saline (pH 7.0) and then lysed in an ice-cold cell lysis buffer containing protease and phosphatase inhibitors. Cellular lysates were spun, supernatants were recovered, and the total protein concentration was determined by protein assay (Bio-Rad). For immunoblotting, 30 or 50 μg of total lysate in 2× SDS-PAGE sample buffer (1:1, v/v) were electrophoresed and transferred to a nitrocellulose membrane. Membranes were incubated with the appropriate primary antibody in TBS-T (pH 7.5) and 5% skim milk or 5% bovine serum albumin at 4°C overnight. After rinsing, the membrane was incubated with secondary antibody in TBS-T buffer for 1 hour. Protein bands were visualized by SuperSignal (Thermo Scientific). For reblotting, filters were agitated with the stripping buffer [62.5 mmol/L Tris (pH 6.8), 2% SDS, 100 mmol/L β-mercaptoethanol] for 30 minutes at 60°C. After two washes with TBS-T buffer, filters were treated with specific primary antibody followed by the corresponding secondary antibody, and the signal was detected by SuperSignal. All immunoblot experiments were conducted three times, and representative results are shown.

Immunofluorescence

Subcellular localization of Smad3 and phospho-Smad3 in parental and cyclin D1–overexpressing cells was determined by indirect immunofluorescence using an anti-Smad3 or anti–phospho-Smad3 antibody. After fixation with 4% paraformaldehyde, slides were incubated with anti-Smad3 antibody at 4°C for 16 hours. Slides were washed three times with TNT buffer [0.1 mol/L Tris-HCl (pH 7.5), 0.15 mol/L NaCl, 0.05% Tween 20]. After 30 minutes of incubation at room temperature with secondary anti-rabbit horseradish peroxidase–conjugated antibody, slides were incubated with fluorophore tyramide (Perkin-Elmer) for 10 minutes. After mounting the slides with Vectashield mounting medium (Vector Laboratories, Inc.) containing a 4′,6-diamidino-2-phenylindole (DAPI) nuclear stain, the cells were observed with a Leica microscope (Leica Microsystems, Inc.) equipped with an oil immersion 40× lens. Digital images were collected using filters for fluorescein and DAPI.

CDK kinase assays

Cell extracts were obtained by lysing cells in lysis buffer [50 mmol/L HEPES (pH 7.0), 250 mmol/L NaCl, 5 mmol/L EDTA (pH 8.0), 0.5% NP40, 1 mmol/L phenylmethylsulfonyl fluoride, 1 mmol/L sodium vanadate, 1× Halt Protease Inhibitor Cocktail (Pierce)] on ice for 30 minutes with occasional agitation. Cell debris was removed by centrifugation at 14,000 × g for 10 minutes at 4°C. Protein concentration was determined using the Bio-Rad protein assay. Protein lysate (50 μg) was incubated with 2 μg of anti-CDK4 or anti-CDK2 IgG (Santa Cruz Biotechnology) at 4°C for 1 hour followed by immunoprecipitation with protein A/G plus agarose conjugate (Santa Cruz Biotechnology) at 4°C overnight. Beads were washed three times with kinase buffer [8 mmol/L MOPS (pH 7.0), 0.2 mmol/L EDTA]. The CDK4 or CDK2 kinase reactions were done at 30°C for 30 minutes in kinase buffer containing 2 μg of recombinant Rb protein or histone H1 (Millipore) as substrate for CDK4 and CDK2, respectively, and 2 μCi [γ-32P]ATP. The reaction was stopped by adding 5× SDS loading buffer and boiled for 5 minutes before loading on a 10% SDS-PAGE gel. The gel was then exposed to a phosphor screen for 24 hours and analyzed using a Storm 860 Molecular Imager (GE Healthcare). Quantitative analysis was done with MultiGauge software (FujiFilm).

Transfection and luciferase assays

Smad3 expression plasmids have been described previously and contain individual site mutations (T8, T178, S203, S207, or S212) or multiple site mutations [3M (T8/T178/S212), 4M (T178/S203/S207/S212), and 5M (T8/T178/S203/S207/S212); ref. 18]. The Smad3 mutants were a gift from Dr. Fang Liu (Rutgers, State University of New Jersey, Piscataway, NJ). A CS2 vector control was also used. DNA transfection experiments were done using Lipofectamine 2000 (Invitrogen). Approximately 5.5 × 104 cells were seeded into 48-well plates 24 hours before transfection. Smad3-responsive promoter firefly luciferase-reporter construct (200 ng; CAGA-luc) and control reporter construct (10 ng; pRenilla) were cotransfected with 200 ng of Smad3 expression plasmid. The cells were lysed with passive lysis buffer (Promega) for dual-luciferase assay 48 hours after transfection. Luciferase activity was measured by a Synergy2 luminometer (BioTek Instruments, Inc.), and firefly luciferase activity was normalized to Renilla luciferase activity. Representative means ± SD were obtained from three independent experiments.

Real-time reverse transcription-PCR

Levels of mRNA for c-myc, p15INK4, and p21 were determined by real-time quantitative reverse transcription-PCR (RT-PCR) using PerfeCta SYBR Green Fast Mix (Quanta Bioscience). Total RNA was isolated from cells using the RNeasy Mini kit (Qiagen). Amplification of the samples (1 μg of total RNA per reaction) was carried out using qScript cDNA Super Mix (Quanta Bioscience). All amplifications were run on a 7900HT Fast Real-Time PCR System (Applied Biosystems) using the following conditions: initial denaturation, 95°C for 15 minutes, followed by 40 cycles at 95°C for 1 second and 60°C for 30 seconds. Gene expression was analyzed in terms of the threshold cycle (Ct) normalized to GAPDH (ΔCt). ΔCt values were then compared between control samples and transfected cells to calculate ΔΔCt. Final comparison of transcript ratios between samples was given as 2−ΔΔCt. Representative means ± SD were obtained from three replicates of three independent experiments.

RNA interference

Transfection of cdk4 small interfering RNA (siRNA; Thermo Scientific) was carried out 24 hours after plating cells in a 96-well plate. Cells were incubated overnight with the transfection mix containing 12.5 pmol/L siRNA and 0.25 μL DharmaFECT Transfection Reagent (Thermo Scientific) in Opti-MEM medium (Invitrogen). Transfection of reporter constructs and Smad expression plasmids was carried out as described above. The cells were lysed with passive lysis buffer (Promega) for dual-luciferase assay at 48 hours after transfection. Luciferase activities were measured as described above. Means ± SD were obtained from three replicates of a representative experiment.

Treatment with CDK inhibitors

After transfection, the cells were placed in medium and treated with CDK4 inhibitor II (IC50 value of 200 nmol/L) or CDK2 inhibitor II (IC50 value of 60 nmol/L; Calbiochem) for 48 hours. Based on the IC50 for each inhibitor, the concentrations of the CDK2 and CDK4 inhibitors used in our proposed studies were selected to induce specific CDK2 and CDK4 inhibition. Control cells were maintained in complete medium and treated with solvent alone. All experiments were done in triplicate.

Fluorescence-activated cell sorting and cell cycle analysis

For flow cytometric analysis, cells were plated at a density of 8 × 105 per well in six-well plates. Cells were harvested 48 hours after transfection, washed once with PBS, fixed in 70% cold ethanol, and incubated for 30 minutes at 4°C in PBS containing 100 μg/mL of RNase A and 50 μg/mL of propidium iodide. Cells were loaded into a FACScan flow cytometer (Becton Dickinson) for cell cycle analysis. Flow cytometric analysis was done for at least 20,000 individual events per reaction. Distribution of cells in the three phases of the cell cycle is represented by percentage. Representative results reflect the trends observed in three separate experiments.

Statistical analysis

Statistical procedures for P value analysis were done by Student's t test with two populations to determine the significance of comparisons. P ≤ 0.05 was considered statistically significant.

Characterization of cyclin D1–overexpressing MCF7 and T47D breast cancer cell lines

The study panel of cells included MCF7 and T47D parental, vector control, and cyclin D1–overexpressing (CD1) breast cancer cell lines. The MCF7 cell line is sensitive to both activin and TGFβ, whereas the T47D cell line is responsive only to activin (27). Immunoblotting for cyclin D1 confirmed that the MCF7-CD1 and T47D-CD1 lines expressed the highest amount of this protein relative to the parental and control cells (Fig. 1A). Protein expression of Smad3, phospho-Smad3, CDK2, and CDK4 was similar across the parental, vector control, and CD1 lines. Kinase assays were done to measure the relative amounts of CDK4 and CDK2 activity in the study cells. As expected, the MCF7-CD1 and T47D-CD1 cells showed the highest amount of CDK4 activity relative to the parental and vector control–transfected cells (Fig. 1B). No difference in CDK2 activity was found among the study cells (Fig. 1C). To determine the subcellular localization of Smad3 in the study panel of cells, immunofluorescence was done using an anti-Smad3 or anti–phospho-Smad3 antibody. Immunofluorescent staining for Smad3 and phospho-Smad3 showed that the MCF7 (Fig. 2A and B) and T47D (Fig. 2C and D) study cells contained both cytoplasmic and nuclear Smad3. Importantly, the study cells designed to overexpress cyclin D showed the presence of cytoplasmic and nuclear Smad3, helping to exclude compromise of nucleocytoplasmic shuttling in these cells as a cause for the decreased Smad3 activity found in this setting. Although variations in nucleocytoplasmic shuttling of Smad3 may contribute to the level of Smad3 activity in a given cell line, overall, each of the six cell lines in the study panel showed the capacity for nuclear translocation of Smad3.

FIGURE 2.

Smad3 (A, C) and phospho-Smad3 (B, D) localization in cyclin D–overexpressing MCF7 and T47D cells. Smad3 and phospho-Smad3 localized to the nucleus in MCF7 (A and B) and T47D (C and D) parental, vector control (V), and cyclin D–overexpressing (CD1) cell lines. Endogenous Smad3 and phospho-Smad3 were visualized by immunofluorescence microscopy with an anti-Smad3 polyclonal antibody and FITC-conjugated secondary antibody. Cell nuclei were counterstained with DAPI. Scale bar, 10 μm. Arrows, nuclei; arrowheads, cytoplasmic Smad3.

FIGURE 2.

Smad3 (A, C) and phospho-Smad3 (B, D) localization in cyclin D–overexpressing MCF7 and T47D cells. Smad3 and phospho-Smad3 localized to the nucleus in MCF7 (A and B) and T47D (C and D) parental, vector control (V), and cyclin D–overexpressing (CD1) cell lines. Endogenous Smad3 and phospho-Smad3 were visualized by immunofluorescence microscopy with an anti-Smad3 polyclonal antibody and FITC-conjugated secondary antibody. Cell nuclei were counterstained with DAPI. Scale bar, 10 μm. Arrows, nuclei; arrowheads, cytoplasmic Smad3.

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Cyclin D modulates Smad3 transcriptional activity

The MCF7 and T47D breast cancer cell lines were transfected with WT Smad3, vector control, or the Smad3 5M CDK phosphorylation site mutant, and the expression levels of p15INK4B, p21, and c-myc were determined by real-time quantitative RT-PCR (Fig. 3A and B). Parental and control MCF7 and T47D cells transfected with the WT Smad3 or Smad3 5M constructs showed lower levels of c-myc transcripts compared with study cells transfected with the vector control. Conversely, parental and control MCF7 and T47D cells transfected with the WT Smad3 and Smad3 5M constructs had higher amounts of p15INK4B and p21 transcripts when compared with cells transfected with the vector control. As expected, the cyclin D–overexpressing lines transfected with the control vector had the highest amounts of c-myc and lowest amounts of p15INK4B transcripts. When these cells were transfected with WT Smad3 or Smad3 5M, c-myc mRNA levels were lower and p15INK4B mRNA levels were higher than in the controls. Of note, the effect of WT Smad3 or 5M Smad3 overexpression on c-myc and p15INK4B transcript levels was more pronounced in T47D cells than in MCF7 cells. In addition, p21 transcript levels remained high in MCF7-CD1 cells and low in T47D-CD1 cells, regardless of WT Smad3 or Smad3 5M overexpression. These data suggest that in parental breast cancer cells, restoration of Smad3 function by overexpression of either WT Smad3 or the Smad3 5M CDK phosphorylation site mutant resulted in lower c-myc expression and higher CDK inhibitor expression. In breast cancer cells that overexpress cyclin D1, restoration of Smad3 function also resulted in relatively lower c-myc and higher p15INK4B expression; however, expression levels of p21 were not affected.

FIGURE 3.

Expression of Smad3-regulated genes in study cell lines. MCF7 (A) and T47D (B) cell lines were transfected with WT Smad3 or the 5M Smad3 CDK phosphorylation site mutant, and transcript levels of c-myc, p15, and p21 were measured by real-time quantitative RT-PCR.

FIGURE 3.

Expression of Smad3-regulated genes in study cell lines. MCF7 (A) and T47D (B) cell lines were transfected with WT Smad3 or the 5M Smad3 CDK phosphorylation site mutant, and transcript levels of c-myc, p15, and p21 were measured by real-time quantitative RT-PCR.

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Abrogation of Smad3 phosphorylation by CDK increases transcriptional activity in MCF7 and T47D cells

Transfection experiments were done to determine the transcriptional activity of the various Smad3 CDK phosphorylation site mutant constructs in the MCF7 (Fig. 4A) and T47D (Fig. 4B) study cells. An additional estrogen receptor–negative breast cancer cell line, Hs578T (Fig. 4C), was also examined. The Hs578T cell line is sensitive to TGFβ signaling (27). Study cells were cotransfected with each of the Smad3 expression plasmids, the Smad-responsive CAGA-luc reporter, and a pRenilla luciferase construct. Compared with WT Smad3, overexpression of the Smad3 T178 mutant in the MCF7 and Hs578T cell lines, and the Smad3 T8 mutant in the T47D cell lines, resulted in relatively higher CAGA-luc reporter activity. For all the study cell lines, overexpression of the Smad3 4M and Smad3 5M constructs also showed high reporter activity. Based on these experiments, the Smad3 T178 mutant was chosen for further study in the MCF7 and Hs578T cell lines and the Smad3 T8 mutant was chosen for further study in the T47D cell lines. The Smad3 5M construct was also further examined in all study cell lines.

FIGURE 4.

Relative transcriptional activity of various Smad3 constructs in cyclin D1–overexpressing MCF7 (A), T47D (B), and Hs578T (C) cell lines. Cells were cotransfected with the Smad3-responsive CAGA-luc reporter construct and Renilla luciferase reporter, in addition to the indicated Smad3 expression constructs. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7, T47D, or Hs578T cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

FIGURE 4.

Relative transcriptional activity of various Smad3 constructs in cyclin D1–overexpressing MCF7 (A), T47D (B), and Hs578T (C) cell lines. Cells were cotransfected with the Smad3-responsive CAGA-luc reporter construct and Renilla luciferase reporter, in addition to the indicated Smad3 expression constructs. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7, T47D, or Hs578T cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

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CDK4 inhibition restores Smad3 activity in breast cancer cell lines

To examine the direct effect of CDK inhibition on Smad3-responsive reporter activity in all MCF7 (Fig. 5A) and T47D (Fig. 5B) cell lines, the cells were transfected with WT Smad3 expression vector and the CAGA-luc and pRenilla reporter constructs. The cells were then treated with increasing concentrations of CDK2 and CDK4 inhibitors. Treatment with escalating doses of the CDK2 inhibitor resulted in a small increase in Smad3 reporter activity for the MCF7 cells, although no significant increase in reporter activity was found for the T47D-treated cells. Furthermore, we did not see a great increase in Smad3 reporter activity when we tested higher concentrations of the CDK2 inhibitor (400 and 800 nmol/L), although a slight increase found in cells treated with 800 nmol/L inhibitor may be attributed to the ability of this CDK2 inhibitor to also act against CDK1, which has an IC50 value of 760 nmol/L and would be affected at this concentration (data not shown). A dose-dependent increase in Smad3 transcriptional activity was seen in all six MCF7 and T47D cell lines treated with increasing concentrations of the CDK4 inhibitor. Thus, Smad3 transcriptional activity could be enhanced through inhibition of CDK4, including cells overexpressing cyclin D1.

FIGURE 5.

Dose-dependent increase in Smad3 transcriptional activity in MCF7 and T47D cells treated with increasing concentrations of CDK2 or CDK4 inhibitors. MCF7 (A) or T47D (B) study cell lines were transfected with the Smad3-responsive CAGA-luc reporter construct, Renilla luciferase reporter, and WT Smad3 expression vector and then treated with the indicated concentrations of the CDK2 inhibitor (CDK2i) or the CDK4 inhibitor (CDK4i). Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7 or T47D cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

FIGURE 5.

Dose-dependent increase in Smad3 transcriptional activity in MCF7 and T47D cells treated with increasing concentrations of CDK2 or CDK4 inhibitors. MCF7 (A) or T47D (B) study cell lines were transfected with the Smad3-responsive CAGA-luc reporter construct, Renilla luciferase reporter, and WT Smad3 expression vector and then treated with the indicated concentrations of the CDK2 inhibitor (CDK2i) or the CDK4 inhibitor (CDK4i). Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7 or T47D cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

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To further examine the combined effect of CDK4 inhibition and abrogation of CDK phosphorylation of Smad3 on Smad3 transcriptional activity, MCF7 (Fig. 6A), T47D (Fig. 6B), and Hs578T (Fig. 6C) parental, vector control, and cyclin D1–overexpressing cells were transfected with Smad3 WT or Smad3 mutant constructs, the CAGA-luc reporter, and the pRenilla reporter, and then treated with vehicle or 800 nmol/L CDK4 inhibitor. As seen previously, when compared with WT Smad3, transfection with the Smad3 T178, Smad3 T8, or Smad3 5M CDK phosphorylation site mutants resulted in higher CAGA-luc reporter activity. Cells transfected with the Smad3 T178 or Smad3 T8 mutants and treated with the CDK4 inhibitor further increased CAGA-luc reporter activity, including the cyclin D1–overexpressing cell lines. Interestingly, transfection with the Smad3 5M mutant and treatment with the CDK4 inhibitor resulted in decreased CAGA-luc reporter activity in MCF7 and Hs578T cells and abolished CAGA-luc reporter activity in T47D cells. This finding suggests that some amount of CDK4 activity may be required for Smad3 signaling.

FIGURE 6.

Restoration of Smad3 transcriptional activity with inhibition of CDK4 activity. MCF7 (A), T47D (B), and Hs578T (C) study cell lines were transfected with the Smad3-responsive CAGA-luc reporter construct, Renilla luciferase reporter, and either WT Smad3, 5M Smad3, T178 Smad3 (MCF7 and Hs578T), or T8 Smad3 (T47D only) expression vectors. The cells were treated with vehicle or 800 nmol/L CDK4 inhibitor. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7, T47D, or Hs578T cells. Columns, mean normalized luciferase activity for each study condition; bars, SD. Asterisk denotes value too low to graphically represent.

FIGURE 6.

Restoration of Smad3 transcriptional activity with inhibition of CDK4 activity. MCF7 (A), T47D (B), and Hs578T (C) study cell lines were transfected with the Smad3-responsive CAGA-luc reporter construct, Renilla luciferase reporter, and either WT Smad3, 5M Smad3, T178 Smad3 (MCF7 and Hs578T), or T8 Smad3 (T47D only) expression vectors. The cells were treated with vehicle or 800 nmol/L CDK4 inhibitor. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7, T47D, or Hs578T cells. Columns, mean normalized luciferase activity for each study condition; bars, SD. Asterisk denotes value too low to graphically represent.

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siRNA knockdown of CDK4 restores Smad3 activity in MCF7 cell lines

To further explore the effect of CDK4 on Smad3 transcriptional activity, MCF7 study cells were transfected with scrambled or cdk4-specific siRNA. The effect of CDK4 inhibition was similar in both sets of study cells; thus, MCF7 cells were selected for subsequent knockdown experiments. MCF7 cells transfected with cdk4 siRNA showed a 70% decrease in CDK4 levels compared with cells treated with a control vector or scrambled siRNA, thus showing the specificity of the cdk4 siRNA knockdown (Fig. 7A). Subsequent cotransfection of the MCF7 study panel of cells with the cdk4 siRNA, WT Smad3, and the Smad3-responsive CAGA-luc reporter resulted in increased reporter activity in the MCF7 parental and vector control cells (Fig. 7B). This increase was not seen in the cyclin D–overexpressing MCF7-CD1 cells, where transfection of cdk4 siRNA was not sufficient to enhance Smad3 activity. Cotransfection of the study cells with cdk4 siRNA and the Smad3 T178 CDK phosphorylation site mutant also resulted in an increase in CAGA-luc reporter activity above that seen in MCF7 parental and vector control cells containing control vector or scrambled siRNA. Although less pronounced, an increase in reporter activity was also seen in the MCF7-CD1 cells cotransfected with cdk4 siRNA and the Smad3 178V construct, suggesting that the high cyclin D1 levels in these cells maintained suppression of Smad3 activity. These data support a direct role of CDK4 in the inhibition of Smad3 action in breast cancer cells.

FIGURE 7.

Restoration of Smad3 transcriptional activity with siRNA knockdown of CDK4. A, MCF7 cells were transfected with scrambled (SC) or cdk4 siRNA for 48 h, and then the cells were lysed and the level of CDK4 protein was determined in untransfected (UC) and transfected cells by immunoblot analysis using anti-CDK4 antibody. GAPDH was used as loading control. B, MCF7 study cell lines were cotransfected with the Smad3-responsive CAGA-luc reporter construct and Renilla luciferase reporter; siRNA or cdk4 siRNA; and either empty vector, WT Smad3, or T178 Smad3 mutant expression vectors. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7 cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

FIGURE 7.

Restoration of Smad3 transcriptional activity with siRNA knockdown of CDK4. A, MCF7 cells were transfected with scrambled (SC) or cdk4 siRNA for 48 h, and then the cells were lysed and the level of CDK4 protein was determined in untransfected (UC) and transfected cells by immunoblot analysis using anti-CDK4 antibody. GAPDH was used as loading control. B, MCF7 study cell lines were cotransfected with the Smad3-responsive CAGA-luc reporter construct and Renilla luciferase reporter; siRNA or cdk4 siRNA; and either empty vector, WT Smad3, or T178 Smad3 mutant expression vectors. Firefly and Renilla luciferase activities were determined. Data are shown as fold increase in normalized luciferase activity (firefly/Renilla) compared with empty vector–transfected MCF7 cells. Columns, mean normalized luciferase activity for each study condition; bars, SD.

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Smad3 overexpression and CDK4 inhibition increase G1 cell cycle distribution

To study the effect of CDK4 inhibition on Smad3 on cell cycle control, the MCF7 study cell lines were transfected with either WT Smad3 or the Smad3 T178 CDK phosphorylation site mutant and treated with the CDK4 inhibitor or vehicle alone. T47D study cell lines were transfected with either WT Smad3 or the Smad3 T8 mutant and treated with the CDK4 inhibitor or vehicle control. Cells were harvested and cell cycle profiles were assessed. MCF7 parental cells had a baseline G1 population of 82.2% (Fig. 8A). This increased to 88.6% after treatment with the CDK4 inhibitor, irrespective of WT Smad3 or Smad3 T178 overexpression. By comparison, MCF7-CD1 cells had a lower baseline G1 population (55.1%) compared with the parental line and had the highest number of cells in the G1 population on Smad3 T178 mutant overexpression and treatment with the CDK4 inhibitor (79.0%).

FIGURE 8.

Inhibition of CDK4-mediated phosphorylation of Smad3 leads to G1 arrest in MCF7 parental and cyclin D–overexpressing cell lines. A, MCF7 and MCF7-CD1 cells were transfected with empty vector (V), WT Smad3 (S), or the T178 Smad3 mutant expression vectors. B, T47D and T47D-CD1 cells were transfected with empty vector, WT Smad3, or the T8 Smad3 mutant expression vectors. The cells were then treated with vehicle or 800 nmol/L CDK4 inhibitor (I). Cells were harvested and the cell cycle profile was assessed by fluorescence-activated cell sorting analysis. Figures show one representative experiment from three separate data sets.

FIGURE 8.

Inhibition of CDK4-mediated phosphorylation of Smad3 leads to G1 arrest in MCF7 parental and cyclin D–overexpressing cell lines. A, MCF7 and MCF7-CD1 cells were transfected with empty vector (V), WT Smad3 (S), or the T178 Smad3 mutant expression vectors. B, T47D and T47D-CD1 cells were transfected with empty vector, WT Smad3, or the T8 Smad3 mutant expression vectors. The cells were then treated with vehicle or 800 nmol/L CDK4 inhibitor (I). Cells were harvested and the cell cycle profile was assessed by fluorescence-activated cell sorting analysis. Figures show one representative experiment from three separate data sets.

Close modal

Parental T47D cells had a baseline G1 population of 68.4%, which increased to 85.8% in T47D cells overexpressing the Smad3 T8 mutant and treated with the CDK4 inhibitor (Fig. 8B). T47D-CD1 cells had a baseline G1 population of 47.6% compared with 79.0% for T47D-CD1 cells transfected with the Smad3 T8 mutant and treated with the CDK4 inhibitor. These data support the hypothesis that inhibition of CDK4-mediated phosphorylation of Smad3, by eliminating the Smad3 phosphorylation sites and through treatment with the CDK4 inhibitor, restores Smad3 activity and cell cycle control in breast cancer cells, including those overexpressing cyclin D1.

The goal of this work was to examine the effect of cyclin D1 overexpression and CDK4 phosphorylation on Smad3 activity in breast cancer cells. A correlation between CDK4 inhibition and restoration of Smad3 function was established. Overexpression of cyclin D1 repressed WT Smad3 transcriptional activity, and this activity was rescued with the overexpression of Smad3 containing single or multisite mutations at CDK phosphorylation sites. Direct inhibition of CDK4 also restored Smad3 transcriptional activity, and this effect was further augmented by overexpressing Smad3 containing mutated CDK phosphorylation sites. Transfection of cyclin D1–overexpressing breast cancer cells with Smad3 T178 and T8 CDK phosphorylation site mutants and treatment with a CDK4 inhibitor resulted in a significant increase in the G1 cell cycle population. Taken together, these data support our hypothesis that cell cycle control is regulated, in part, by Smad3, and that the growth-suppressive effect of Smad3 is lost on CDK4 phosphorylation of Smad3 in cyclin D1–overexpressing breast cancer cells.

Previous work has examined the role of Smad3 in cell cycle regulation. Smad3, acting in conjunction with both cytoplasmic and nuclear cofactors, has been linked to the transcription of CDK inhibitors p15 and p21 and the inhibition of mitogenic c-myc in several different cell lines, including breast cancer cells (7, 8, 28). Furthermore, Smad3 overexpression in T47D breast cancer cells was shown to induce cell cycle arrest and expression of the CDK inhibitor p15, as well as repress cyclin A expression and Rb phosphorylation (29). The current study adds to the mechanistic understanding of these observations through the examination of Smad3 constructs with CDK mutation sites in breast cancer cell lines overexpressing cyclin D1. Notably, in the parental cells used in the study, c-myc transcript levels decreased after transfection with WT Smad3, and this decrease was significantly augmented by transfection of the 5M Smad3 construct. In the study cells overexpressing cyclin D1, the effect of transfection of the 5M Smad3 construct on c-myc repression and p15 transcription was even more pronounced. This finding supports a repressive effect of cyclin D1 overexpression on Smad3 action in the breast cancer cell lines and also confirms previous findings of the role of Smad3 in the regulation of c-myc repression and p15 transcription (10, 30).

In contrast to p15 expression, p21 transcript levels were not affected by overexpression of the 5M Smad3 CDK phosphorylation site mutant in cyclin D1–overexpressing breast cancer cells in our study. Whereas both TGFβ and BMP ligand subgroups within the TGFβ superfamily facilitate p21 transcription, BMP-related Smad signaling is associated with higher p21 expression levels than signaling through TGFβ/activin (31). On the other hand, although the BMP-specific Smads induce p21 mRNA and protein expression, this induction does not result in epithelial growth inhibition as seen with TGFβ/activin-specific Smad signaling (31). Importantly, these data suggest that although transcription of p21 is associated with several members of the TGFβ superfamily, additional cofactors or signaling targets must also be involved to facilitate cell growth arrest (31). Serum response factor (SRF) has recently been associated with cancer progression and metastasis, specifically as an inhibitor of Smad3-mediated transcription of p15 and p21 (32). It has been proposed that SRF acts at the nuclear level through association with the Smad3/4 complex to inhibit binding to and transcription of Smad-responsive genes (32). Potentially, the presence or absence of SRF in certain breast cancer settings may contribute to the loss of Smad-mediated cell cycle control potentiated by CDK phosphorylation. The role of additional cofactors involved in cross-talk with TGFβ/activin-specific Smad signaling to regulate cell cycle entry will be examined in future studies.

Of note, Smad3 activity was restored most effectively with overexpression of the 5M Smad3 CDK phosphorylation site mutant in the MCF7-CD1 and Hs578T-CD1 cell lines and by overexpression of the 4M or 5M Smad3 mutants in T47D-CD1 cells. Thus, cyclin D/CDK-mediated Smad3 repression is most effectively overcome through mutation of most or all CDK phosphorylation sites within the protein. In light of these findings, CDK inhibitors that block CDK2 and CDK4 phosphorylation at the Smad3 mutation sites were examined for their ability to restore Smad3 action. In both MCF7 and T47D study cell lines, CDK2 inhibition resulted in a slight, if any, increase in Smad3 activity above that seen with overexpression of WT Smad3, whereas CDK4 inhibition resulted in a significant increase in Smad3 transcriptional activity. Thus, CDK2 phosphorylation seems to play a minor role in Smad3 inhibition in MCF7 cells and no appreciable role in T47D cells. Our subsequent experiments silencing CDK4 activity, either through overexpression of Smad3 mutants containing phosphorylation site mutations or through treatment with the CDK4 inhibitor, confirmed the effect of CDK4 inhibition on restoring Smad3 transcriptional activity. We expected that maximal inhibition of the CDK4 effect on Smad3 activity would be achieved with transfection of the 5M Smad3 mutant in addition to treatment with a CDK4 inhibitor. However, this led to reporter activity that was slightly lower than that seen in MCF7-CD1 and Hs578T-CD1 cells transfected with the 5M construct alone and to near-complete abrogation of reporter activity in the T47D-CD1 cells.

The transcriptional activity of Smad3 is modulated by the binding of cofactors such as p300/CBP (33). Competitive binding of p300/CBP between signal transducer and activator of transcription 1α (STAT1α), a component of the Janus-activated kinase–STAT pathway, and Smad3 has been described as a mechanism involved in regulation of collagen transcription in fibroblasts (34). In conjunction with p300/CBP, the PIAS3 protein, from the protein inhibitor of activated STAT family, may also modulate TGFβ-mediated Smad3 transcriptional activity (35). p300/CBP binding to Smad3 takes place within the linker region of the Smad3 molecule and may be affected by CDK phosphorylation in this region (36). Likewise, the presence or absence of CDK phosphorylation within the Smad3 linker region may affect the capacity for binding of Smad3 to various corepressors or coactivators, including STAT1α or PIAS3; this may represent a mechanism for cyclin-mediated phosphorylation inhibition of Smad3 activity (19). On the other hand, p300/CBP binding to Smad3 may require some level of CDK activity in T47D cells, which may explain why Smad3 transcriptional activity was completely abolished by overexpression of the 5M Smad3 mutant and treatment with the CDK4 inhibitor. Recent data from myeloma cells found that phosphorylation of Smad2 at the T8 site by CDK2 prevented Smad2 from linking with the co-Smad Smad4, thus inhibiting Smad-dependent transcriptional activity (37). In our breast cancer cell studies, however, mutation of the T8 site proved significant for restoring Smad3 activity in T47D cells, although less so in MCF7 and Hs578T cells. At minimum, these data point toward a dual significance of CDK phosphorylation of Smads in different malignant settings and the potential for certain CDK sites to be critical for Smad interaction with cofactors and coregulators important for transcriptional activity (37).

Previous work has shown that the mean tumor size in patients with moderate to intense nuclear Smad3 breast cancer tissue staining was ∼1.5 cm smaller than in those patients with low or no nuclear Smad3 staining (17). The correlation between nuclear Smad3 and smaller tumor size implicates activated and functional nuclear Smad3 in the inhibition of breast tumor cell proliferation. Tumor size, a component of the American Joint Committee on Cancer Staging System for breast cancer, is one of the most powerful predictors of breast cancer prognosis, with smaller tumors having a more favorable outcome. As nuclear Smad3 staining intensity has shown an independently significant correlation with smaller tumor size, it may also have favorable prognostic significance (17). Our data support the use of Smad3 as a prognostic marker in conjunction with cyclin expression, as tumors with activated nuclear Smad3, but with high cyclin activity, may have lost Smad3-mediated cell cycle control as a consequence of CDK phosphorylation. Tian et al. (16) have shown in a mouse model that tumors formed from MCF-10A cells overexpressing Smad3 grew more slowly than MCF-10A cells overexpressing a Smad3 dominant-negative mutant. Likewise, the current study showed that breast cancer cells overexpressing Smad3 with CDK phosphorylation site mutations could restore cell cycle control and G1 arrest even in the presence of high levels of cyclin D1. The significance of these findings further reveals how Smad3-mediated cell cycle control can be undermined in breast cancers that overexpress cyclin D and restored by blockade of Smad3 CDK phosphorylation.

The possibility of targeting CDKs for therapeutic benefit is being pursued. Three classes of CDK inhibitors have been designed: agents that affect several CDKs simultaneously, agents that target individual CDKs, and agents that inhibit both CDK activity as well as other kinase targets (38). Phase 1 and 2 trials have been pursued to study the effect of CDK2 and CDK4 inhibitors, such as flavopiridol, which blocks CDK1, CDK2, CDK4, CDK6, CDK7, and CDK9, on solid and hematogenous malignancies (39, 40). Early results from breast cancer studies examining the effect of flavopiridol in combination with trastuzumab, histone deacetylase inhibitors, and docetaxel seem promising, with the treatment regimen leading to decreases in tumor cell proliferation and tumor size (39, 41, 42). Additionally, work on the blockade of AP-1 in MCF7 breast cancer cells has resulted in cell growth arrest in the G1 phase of the cell cycle and was associated with a reduced expression of cyclins D and E, decreased CDK2/4 activity, and increased p27 expression (43). These data point toward a potential role for targeted CDK inhibitors in breast cancer therapy (43). To date, these agents have not been studied in the context of cyclin-overexpressing breast cancers or Smad3 signaling. In this work, treatment of cyclin D1–overexpressing cells with a CDK4 inhibitor resulted in a dose-dependent increase in Smad3 transcriptional activity; in this setting, CDK4 inhibitor treatment seemed to be more effective at restoring Smad3 activity than CDK2 inhibitor treatment. This finding supports a more selective approach to the development of therapeutic CDK inhibitors to maximize treatment effectiveness and minimize comorbidity.

This study focuses on the effect of cyclin D1 overexpression on Smad3 action in breast carcinogenesis. Breast cancers that overexpress cyclins have been associated with poor prognosis (44-46). A clear understanding of the mechanisms underlying Smad3-mediated cell cycle arrest is crucial to efforts aimed at preventing or interrupting oncogenic insults to the Smad3 signaling pathway that favor breast cancer growth and dedifferentiation. Furthermore, knowledge of the mechanisms responsible for cell cycle deregulation characteristic of cancers with high cyclin activity is critical to the discovery of improved treatment strategies for the patients with these tumors. These efforts will ultimately allow for the further development of individualized prognostic markers to help actualize patient-specific treatment strategies. Specifically, strategies that target inhibition of CDKs or block CDK/cyclin activity may hold promise for patients with cyclin-overexpressing breast cancers that currently have a disease subtype with a poor prognosis.

No potential conflicts of interest were disclosed.

We thank Dr. Fang Liu (Rutgers, State University of New Jersey, Piscataway, NJ) for providing the mutant Smad3 constructs and Elizabeth Tarasewicz for her careful reading of the manuscript.

Grant Support: J.S. Jeruss is a Lynn Sage Scholar supported by the American Cancer Society-Illinois Division, the Dixon Foundation, and NIH KL2 and K22 CA138776 research grants.

The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked advertisement in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.

1
Brown
KA
,
Pietenpol
JA
,
Moses
HL
. 
A tale of two proteins: differential roles and regulation of Smad2 and Smad3 in TGF-β signaling
.
J Cell Biochem
2007
;
101
:
9
33
.
2
Yue
J
,
Mulder
KM
. 
Transforming growth factor-β signal transduction in epithelial cells
.
Pharmacol Ther
2001
;
91
:
1
34
.
3
Massague
J
. 
TGF-β signal transduction
.
Annu Rev Biochem
1998
;
67
:
753
91
.
4
Nakao
A
,
Imamura
T
,
Souchelnytskyi
S
, et al
. 
TGF-β receptor-mediated signalling through Smad2, Smad3 and Smad4
.
EMBO J
1997
;
16
:
5353
62
.
5
Matsuura
I
,
Chiang
KN
,
Lai
CY
, et al
. 
Pin1 promotes TGF-β-induced migration and invasion
.
J Biol Chem
2009
;
285
:
1754
64
.
6
Dumont
N
,
Arteaga
CL
. 
Transforming growth factor-β and breast cancer: tumor promoting effects of transforming growth factor-β
.
Breast Cancer Res
2000
;
2
:
125
32
.
7
Chen
CR
,
Kang
Y
,
Siegel
PM
,
Massague
J
. 
E2F4/5 and p107 as Smad cofactors linking the TGFβ receptor to c-myc repression
.
Cell
2002
;
110
:
19
32
.
8
Feng
XH
,
Liang
YY
,
Liang
M
,
Zhai
W
,
Lin
X
. 
Direct interaction of c-Myc with Smad2 and Smad3 to inhibit TGF-β-mediated induction of the CDK inhibitor p15(Ink4B)
.
Mol Cell
2002
;
9
:
133
43
.
9
Pardali
K
,
Kurisaki
A
,
Moren
A
,
ten Dijke
P
,
Kardassis
D
,
Moustakas
A
. 
Role of Smad proteins and transcription factor Sp1 in p21(Waf1/Cip1) regulation by transforming growth factor-β
.
J Biol Chem
2000
;
275
:
29244
56
.
10
Millet
C
,
Zhang
YE
. 
Roles of Smad3 in TGF-β signaling during carcinogenesis
.
Crit Rev Eukaryot Gene Expr
2007
;
17
:
281
93
.
11
Moustakas
A
,
Pardali
K
,
Gaal
A
,
Heldin
CH
. 
Mechanisms of TGF-β signaling in regulation of cell growth and differentiation
.
Immunol Lett
2002
;
82
:
85
91
.
12
Jeruss
JS
,
Santiago
JY
,
Woodruff
TK
. 
Localization of activin and inhibin subunits, receptors and SMADs in the mouse mammary gland
.
Mol Cell Endocrinol
2003
;
203
:
185
96
.
13
Nguyen
AV
,
Pollard
JW
. 
Transforming growth factor β3 induces cell death during the first stage of mammary gland involution
.
Development
2000
;
127
:
3107
18
.
14
Robinson
SD
,
Silberstein
GB
,
Roberts
AB
,
Flanders
KC
,
Daniel
CW
. 
Regulated expression and growth inhibitory effects of transforming growth factor-β isoforms in mouse mammary gland development
.
Development
1991
;
113
:
867
78
.
15
Xie
W
,
Mertens
JC
,
Reiss
DJ
, et al
. 
Alterations of Smad signaling in human breast carcinoma are associated with poor outcome: a tissue microarray study
.
Cancer Res
2002
;
62
:
497
505
.
16
Tian
F
,
DaCosta Byfield
S
,
Parks
WT
, et al
. 
Reduction in Smad2/3 signaling enhances tumorigenesis but suppresses metastasis of breast cancer cell lines
.
Cancer Res
2003
;
63
:
8284
92
.
17
Jeruss
JS
,
Sturgis
CD
,
Rademaker
AW
,
Woodruff
TK
. 
Down-regulation of activin, activin receptors, and Smads in high-grade breast cancer
.
Cancer Res
2003
;
63
:
3783
90
.
18
Matsuura
I
,
Denissova
NG
,
Wang
G
,
He
D
,
Long
J
,
Liu
F
. 
Cyclin-dependent kinases regulate the antiproliferative function of Smads
.
Nature
2004
;
430
:
226
31
.
19
Liu
F
. 
Smad3 phosphorylation by cyclin-dependent kinases
.
Cytokine Growth Factor Rev
2006
;
17
:
9
17
.
20
Ewen
ME
,
Lamb
J
. 
The activities of cyclin D1 that drive tumorigenesis
.
Trends Mol Med
2004
;
10
:
158
62
.
21
Tashiro
E
,
Tsuchiya
A
,
Imoto
M
. 
Functions of cyclin D1 as an oncogene and regulation of cyclin D1 expression
.
Cancer Sci
2007
;
98
:
629
35
.
22
Roy
PG
,
Thompson
AM
. 
Cyclin D1 and breast cancer
.
Breast
2006
;
15
:
718
27
.
23
Yu
Q
,
Geng
Y
,
Sicinski
P
. 
Specific protection against breast cancers by cyclin D1 ablation
.
Nature
2001
;
411
:
1017
21
.
24
Honrado
E
,
Benitez
J
,
Palacios
J
. 
The molecular pathology of hereditary breast cancer: genetic testing and therapeutic implications
.
Mod Pathol
2005
;
18
:
1305
20
.
25
Preobrazhenska
O
,
Yakymovych
M
,
Kanamoto
T
, et al
. 
BRCA2 and Smad3 synergize in regulation of gene transcription
.
Oncogene
2002
;
21
:
5660
4
.
26
Malumbres
M
,
Barbacid
M
. 
Cell cycle, CDKs and cancer: a changing paradigm
.
Nat Rev Cancer
2009
;
9
:
153
66
.
27
Kalkhoven
E
,
Roelen
BA
,
de Winter
JP
, et al
. 
Resistance to transforming growth factor β and activin due to reduced receptor expression in human breast tumor cell lines
.
Cell Growth Differ
1995
;
6
:
1151
61
.
28
Chen
CR
,
Kang
Y
,
Massague
J
. 
Defective repression of c-myc in breast cancer cells: a loss at the core of the transforming growth factor β growth arrest program
.
Proc Natl Acad Sci U S A
2001
;
98
:
992
9
.
29
Burdette
JE
,
Jeruss
JS
,
Kurley
SJ
,
Lee
EJ
,
Woodruff
TK
. 
Activin A mediates growth inhibition and cell cycle arrest through Smads in human breast cancer cells
.
Cancer Res
2005
;
65
:
7968
75
.
30
Liu
F
,
Matsuura
I
. 
Inhibition of Smad antiproliferative function by CDK phosphorylation
.
Cell Cycle
2005
;
4
:
63
6
.
31
Pardali
K
,
Kowanetz
M
,
Heldin
CH
,
Moustakas
A
. 
Smad pathway-specific transcriptional regulation of the cell cycle inhibitor p21(WAF1/Cip1)
.
J Cell Physiol
2005
;
204
:
260
72
.
32
Lee
HJ
,
Yun
CH
,
Lim
SH
, et al
. 
SRF is a nuclear repressor of Smad3-mediated TGF-β signaling
.
Oncogene
2007
;
26
:
173
85
.
33
Inoue
Y
,
Itoh
Y
,
Abe
K
, et al
. 
Smad3 is acetylated by p300/CBP to regulate its transactivation activity
.
Oncogene
2007
;
26
:
500
8
.
34
Ghosh
AK
,
Yuan
W
,
Mori
Y
,
Chen
S
,
Varga
J
. 
Antagonistic regulation of type I collagen gene expression by interferon-γ and transforming growth factor-β. Integration at the level of p300/CBP transcriptional coactivators
.
J Biol Chem
2001
;
276
:
11041
8
.
35
Long
J
,
Wang
G
,
Matsuura
I
,
He
D
,
Liu
F
. 
Activation of Smad transcriptional activity by protein inhibitor of activated STAT3 (PIAS3)
.
Proc Natl Acad Sci U S A
2004
;
101
:
99
104
.
36
Wang
G
,
Long
J
,
Matsuura
I
,
He
D
,
Liu
F
. 
The Smad3 linker region contains a transcriptional activation domain
.
Biochem J
2005
;
386
:
29
34
.
37
Baughn
LB
,
Di Liberto
M
,
Niesvizky
R
, et al
. 
CDK2 phosphorylation of Smad2 disrupts TGF-β transcriptional regulation in resistant primary bone marrow myeloma cells
.
J Immunol
2009
;
182
:
1810
7
.
38
Malumbres
M
,
Pevarello
P
,
Barbacid
M
,
Bischoff
JR
. 
CDK inhibitors in cancer therapy: what is next?
Trends Pharmacol Sci
2008
;
29
:
16
21
.
39
Fornier
MN
,
Rathkopf
D
,
Shah
M
, et al
. 
Phase I dose-finding study of weekly docetaxel followed by flavopiridol for patients with advanced solid tumors
.
Clin Cancer Res
2007
;
13
:
5841
6
.
40
Lin
TS
,
Ruppert
AS
,
Johnson
AJ
, et al
. 
Phase II study of flavopiridol in relapsed chronic lymphocytic leukemia demonstrating high response rates in genetically high-risk disease
.
J Clin Oncol
2009
;
27
:
6012
8
.
41
Nahta
R
,
Trent
S
,
Yang
C
,
Schmidt
EV
. 
Epidermal growth factor receptor expression is a candidate target of the synergistic combination of trastuzumab and flavopiridol in breast cancer
.
Cancer Res
2003
;
63
:
3626
31
.
42
Mitchell
C
,
Park
MA
,
Zhang
G
, et al
. 
Extrinsic pathway- and cathepsin-dependent induction of mitochondrial dysfunction are essential for synergistic flavopiridol and vorinostat lethality in breast cancer cells
.
Mol Cancer Ther
2007
;
6
:
3101
12
.
43
Liu
Y
,
Lu
C
,
Shen
Q
,
Munoz-Medellin
D
,
Kim
H
,
Brown
PH
. 
AP-1 blockade in breast cancer cells causes cell cycle arrest by suppressing G1 cyclin expression and reducing cyclin-dependent kinase activity
.
Oncogene
2004
;
23
:
8238
46
.
44
Naidu
R
,
Wahab
NA
,
Yadav
MM
,
Kutty
MK
. 
Expression and amplification of cyclin D1 in primary breast carcinomas: relationship with histopathological types and clinico-pathological parameters
.
Oncol Rep
2002
;
9
:
409
16
.
45
Keyomarsi
K
,
Tucker
SL
,
Buchholz
TA
, et al
. 
Cyclin E and survival in patients with breast cancer
.
N Engl J Med
2002
;
347
:
1566
75
.
46
Yang
C
,
Trent
S
,
Ionescu-Tiba
V
, et al
. 
Identification of cyclin D1- and estrogen-regulated genes contributing to breast carcinogenesis and progression
.
Cancer Res
2006
;
66
:
11649
58
.