- Research article
- Open Access
Induction by transforming growth factor-β1 of epithelial to mesenchymal transition is a rare event in vitro
Breast Cancer Research volume 6, Article number: R215 (2004)
Transforming growth factor (TGF)-β1 is proposed to inhibit the growth of epithelial cells in early tumorigenesis, and to promote tumor cell motility and invasion in the later stages of carcinogenesis through the induction of an epithelial to mesenchymal transition (EMT). EMT is a multistep process that is characterized by changes in cell morphology and dissociation of cell–cell contacts. Although there is growing interest in TGF-β1-mediated EMT, the phenotype is limited to only a few murine cell lines and mouse models.
To identify alternative cell systems in which to study TGF-β1-induced EMT, 18 human and mouse established cell lines and cultures of two human primary epithelial cell types were screened for TGF-β1-induced EMT by analysis of cell morphology, and localization of zonula occludens-1, E-cadherin, and F-actin. Sensitivity to TGF-β1 was also determined by [3H]thymidine incorporation, flow cytometry, phosphorylation of Smad2, and total levels of Smad2 and Smad3 in these cell lines and in six additional cancer cell lines.
TGF-β1 inhibited the growth of most nontransformed cells screened, but many of the cancer cell lines were insensitive to the growth inhibitory effects of TGF-β1. In contrast, TGF-β1 induced Smad2 phosphorylation in the majority of cell lines, including cell lines resistant to TGF-β1-mediated cell cycle arrest. Of the cell lines screened only two underwent TGF-β1-induced EMT.
The results presented herein show that, although many cancer cell lines have lost sensitivity to the growth inhibitory effect of TGF-β1, most show evidence of TGF-β1 signal transduction, but only a few cell lines undergo TGF-β1-mediated EMT.
Transforming growth factor (TGF)-β1 is a cytokine that is involved in immune suppression, angiogenesis, apoptosis, cell growth, and epithelial to mesenchymal transitions (EMTs) during carcinogenesis [1–7]. TGF-β1 signals through the TGF-β type I (TβRI) and TGF-β type II (TβRII) transmembrane serine/threonine protein kinase receptors.
When TGF-β1 binds TβRII, TβRI is recruited to TβRII, and TβRII phosphorylates and activates the kinase activity of TβRI. Activated TβRI interacts with and phosphorylates a number of proteins, thereby activating many downstream signaling pathways, including the Smad (Sma/Mothers Against Decapentaplegic) pathway. The Smad signaling cascade is initiated by the phosphorylation of Smad2 or Smad3 by TβRI. Phosphorylated Smad2 and Smad3 associate with Smad4 and are translocated to the nucleus, where they modulate transcription of many genes [8–13].
In early tumorigenesis TGF-β1 inhibits the growth of epithelial cells, and insensitivity to this growth inhibitory effect is associated with tumor progression [5, 6]. Transgenic mice expressing a dominant negative TβRII in the epidermis and mammary glands exhibit accelerated tumor formation and malignant conversion [14, 15]. Resistance to the antiproliferative effects of TGF-β1 is observed in head and neck squamous cell carcinomas [16–18], lung cancer , gastric cancer [20–22], colon cancer [22–25], pancreatic cancer , ovarian cancer [27, 28], and in some recurrent breast cancers [29, 30]. This loss of sensitivity to TGF-β1 is due to mutations in or transcriptional repression of the genes that encode TβRI and/or TβRII. Mutations in the genes encoding Smad2 (MADH2) and Smad4 (MADH4) also contribute to the insensitivity to TGF-β1 in many lung , pancreatic , and colorectal [33, 34] carcinomas.
In contrast to the growth inhibitory effects of TGF-β1 in the early stages of carcinogenesis, TGF-β1 can also act as a promoter of tumor cell invasion and metastasis in the later stages of tumorigenesis [5, 6]. Increased production of TGF-β1 is observed in epidermal , gastric , renal , breast [38–41], and prostate carcinomas  when compared with normal tissues. In mice with polyomavirus middle T antigen expression targeted to the mammary gland, blockade of TGF-β1 by administration of Fc:TβRII results in increased apoptosis in primary tumors and reduced tumor cell motility, intravasation, and metastasis . Chronic exposure of mouse epidermal cells to TGF-β1 results in loss of TGF-β1-mediated growth inhibition and marked changes in cell morphology, downregulation of E-cadherin and cytokeratins, upregulation of vimentin, and formation of spindle cell carcinomas in mice [44, 45]. Further studies show that carcinomas with excess TGF-β1 production are more motile and invasive, and exhibit increased tumor cell metastasis in athymic mice [36, 40, 45–51].
One mechanism by which TGF-β1 can promote tumor cell motility and invasion is through the induction of EMT . EMT is a complex process that involves changes in cell morphology and dissociation of cell–cell contacts [53, 54]. Cells undergoing EMT change from a cobblestone-like appearance to an elongated, mesenchymal phenotype. Accompanying this morphologic change is the delocalization of adherens and tight junctional proteins from the cell–cell junctions, and remodeling of the actin cyto-skeleton [53, 54]. Characteristics associated with EMT, such as the dissociation of cell–cell and cell–extracellular matrix contacts, acquisition of an elongated cell morphology, and rearrangement of the cytoskeleton, can facilitate cell migration and invasion [55–57].
Although TGF-β1 is thought to play a key role in EMT in vivo, the frequency of TGF-β1-induced EMT in vitro is not known. To identify alternative cell systems in which to study TGF-β1-mediated EMT, we screened primary cultures of two human epithelial cell types and 18 established mouse and human cell lines for TGF-β1 responsiveness. We also included six additional cancer cell lines as a comparison for TGF-β1 responsiveness. We found that many of the cell strains displayed morphological changes and exhibited actin stress fiber responses to TGF-β1. However, only in the NMuMG and MCT cells were those changes accompanied by a loss of E-cadherin and zonula occludens (ZO)-1 at cell–cell junctions after 48 hours of TGF-β1 treatment. Whereas all of the nontransformed cells were growth inhibited by TGF-β1, many of the cancer cell lines were insensitive to the growth inhibitory effects of TGF-β1. The TGF-β1-mediated growth inhibition was accompanied by an increase in phosphorylated Smad2 protein levels, but this was not unique to growth inhibited cells because changes in Smad2 phosphorylation occurred in a majority of cells after TGF-β1 treatment. In addition, prolonged TGF-β1 treatment induced a decrease in total Smad2 and/or total Smad3 in some cell lines. Our findings show that, although many cancer cells lost sensitivity to the growth inhibitory effect of TGF-β1, only two murine cell lines underwent TGF-β1-mediated EMT and these cells retain growth inhibitory response to TGF-β1.
Cell lines and culture conditions
A549, BT549, DU145, H1299, HBL100, MCF10A, MCF7, MDA-MB-231, MDA-MB-361, MDA-MB-435S, MDA-MB-436, MDA-MB-468, NMuMG, and 4T1 cells were purchased from American Type Culture Collection (Rockville, MD, USA). Primary human epidermal keratinocytes (HEKs) from human infant foreskin were obtained from the Vanderbilt University Skin Disease Research Center. Primary human mammary epithelial cells (HMECs) from two females (#1012 and #1016) were isolated and provided by S Eltom (Meharry Medical College). Mouse keratinocyte (MK) cells were provided by B Weissman (University of North Carolina, Chapel Hill, NC, USA). EpH4 cells were provided by C Arteaga (Vanderbilt University). KC (mouse keratinocytes transformed with K-ras) cells were derived from BALB/MK cells by Kirsten murine sarcoma virus transformation, as described previously . HaCaT cells were provided by P Boukamp (Deutsches Krebsforschungszentrum, Heidelberg, Germany). MCT cells were provided by E Neilson (Vanderbilt University). Panc-1 tumor cells were provided by L Matrisian (Vanderbilt University). Colo357 tumor cells were provided by M Korc (University of California, Irvine, CA, USA). SCC012 and SCC028 cells were provided by D Sidransky (Johns Hopkins University, Baltimore, MD, USA). Finally, UNC10 cells were provided by W Yarbrough (Vanderbilt University).
A549, Colo357, DU145, EpH4, H1299, HaCaT, HBL100, MCT, Panc-1, and 4T1 cells were maintained in Dulbecco's modified Eagle's medium (DMEM)/high-glucose medium (HyClone, Logan, UT, USA) supplemented with 10% fetal bovine serum (FBS). BT549 cells were maintained in RPMI-1640 medium (HyClone) supplemented with 10% FBS and 10 μg/ml insulin. NMuMG cells were maintained in DMEM/high-glucose medium supplemented with 10% FBS and 10 μg/ml insulin. HMEC-1016 and HMEC-1012 were grown in DMEM:F12 medium (1:1) (GibCoBRL, Grand Island, NY, USA) supplemented with 1% FBS, 10 μg/ml ascorbic acid, 2 nmol/l β-estradiol, 35 μg/ml bovine pituitary extract, 1 ng/ml cholera toxin, 12.5 ng/ml epidermal growth factor (EGF), 0.1 mmol/l ethanolamine, 0.1 mmol/l phospho-ethanolamine, 1 μg/ml hydrocortisone, 1 μg/ml insulin, 0.2 mmol/l L-glutamine, 10 nmol/l T3, 10 μg/ml transferrin, and 15 nmol/l sodium selenite.
HEKs were maintained in EpiLife medium supplemented with human keratinocyte growth supplement (S-001-5) and 0.06 mol/l CaCl2 (Cascade Biologics, Portland, OR, USA). MCF-7 cells were maintained in minimal essential medium (MEM; GibCoBRL) supplemented with 10% FBS, 10 μg/ml insulin, 1% nonessential amino acids, and 22 μg/ml sodium pyruvate. MCF10A cells were cultured in (1:1) DMEM:F12 medium (Hyclone) supplemented with 5% horse serum, 100 ng/ml cholera toxin, 20 ng/ml EGF, 500 ng/ml hydrocortisone, and 10 μg/ml insulin. MDA-MB-231, -361, -435S, and -436 cells were maintained in McCoy's 5A medium (HyClone) supplemented with 10% FBS. MDA-MB-468 cells were grown in DMEM/high-glucose:McCoy's 5A medium (1:1) supplemented with 10% FBS. MK and KC cells were maintained in DMEM/high-glucose medium supplemented with 8% dialyzed FBS, 5 μg/ml calcium, and 4 ng/ml EGF. SCC012 and SCC028 cells were maintained in RPMI-1640 medium supplemented with 10% FBS, 1% insulin–transferrin–selenium A, 1% L-glutamine, and 1% non-essential amino acids. UNC10 cells were grown in DMEM/ high-glucose medium supplemented with 10% FBS, 1% insulin–transferrin–selenium A, 1% L-glutamine, and 1% nonessential amino acids.
All cell lines were maintained at 37°C in 5% CO2, except for the NMuMG, MK, and KC cells, which were grown in 7% CO2.
Antibodies and other reagents
TGF-β1 was from R&D Systems (Minneapolis, MN, USA). Antibodies to Smad2/3 (mouse) and E-cadherin (mouse) were from BD Transduction Laboratories (San Diego, CA, USA); antibodies to phosphorylated (Ser 465/467) Smad2 (rabbit lot #21034 and #24432) were from Upstate Biotechnology (Lake Placid, NY, USA); and antibodies to ZO-1 (rat) were from Chemicon International (Temecula, CA, USA). Smad3 (rabbit) and ZO-1 (rabbit ZR-1) antibodies were obtained from Zymed Laboratories Inc. (San Francisco, CA, USA). Anti-actin (rabbit) antibodies and streptavidin–Cy3 conjugate were obtained from Sigma (St. Louis, MO, USA). Rabbit anti-goat, goat anti-mouse, and goat anti-rat biotinylated antibodies were obtained from Vector Laboratories Inc. (Burlingame, CA, USA).
[3H]Thymidine incorporation assays
Subconfluent cells were treated with TGF-β1 (5 ng/ml) for 46 hours in 12-well plates and pulsed for 2 hours with 4 μCi/well [3H]thymidine (Perkin Elmer Life Sciences, Boston, MA, USA). Cells were fixed with 1 ml 10% trichloroacetic acid for 30 min at 25°C, followed by two washes with 10% trichloroacetic acid. DNA was solubilized by incubation in 600 μl 0.2 N NaOH for 30 min, and radioactivity was counted using 200 μl solubilized DNA in 4 ml scintillation fluid.
Flow cytometry analyses
Subconfluent cells were treated with TGF-β1 (5 ng/ml) for 48 hours and approximately 106 cells were incubated in propidium iodide solution (50 μg/ml propidium iodide (Sigma), 5 μg/ml RNase A, 0.1% Triton X-100, and 1 μg/ml sodium citrate) for 5–10 min. Stained cells were analyzed using a FACS Caliber (Becton-Dickinson, San Jose, CA, USA) and the data stored as listmode files. DNA cell cycle histograms were analyzed and modeled using ModFit and WinList software (Verity Software House, Topsham, ME, USA). Fifteen thousand events were analyzed for each sample.
Cell lysis and immunoblot analyses
After 2 hours or 48 hours of treatment with TGF-β1 (5 ng/ml), cells were lysed in protein lysis buffer (50 mmol/l Tris pH 7.5, 100 mmol/l NaCl, 0.5% NP-40, 50 μg/ml PMSF, 4 mmol/l NaF, 0.1 mmol/l Na3VO4) supplemented with protease inhibitors, and protein concentrations in cell lysates were determined using the Bradford method. Protein extracts (100 μg/lane) were separated by 12% SDS-PAGE and transferred to polyvinylidene fluoride membranes (Immobilon-P; Millipore, Bedford, MA, USA). Membranes were blocked in 5% nonfat dry milk in Tris buffered saline with Tween-20 (TTBS; 150 mmol/l NaCl, 100 mmol/l Tris, pH 7.5, 0.1% Tween-20) for 2 hours at 25°C. Membranes to be incubated in phosphorylated Smad2 antibodies lot #24432 were not blocked in milk. Membranes were incubated with primary antibodies diluted in TTBS buffer plus 1% milk (rabbit Smad2 1:1000, phosphorylated Smad2 1:1000 lot #21034 or 1:200 lot #24432, rabbit Smad3 1:300, actin 1:500) for 1 hour or overnight at 4°C for phosphorylated Smad2 lot #24432, washed for 20 min in TTBS buffer, and incubated in secondary antibodies diluted in TTBS buffer plus 1% milk (1:10000) for 1 hour at 25°C. Membranes were washed two times in TTBS buffer (45 min/wash) and immunoreactive bands were visualized by enhanced chemiluminescence.
Subconfluent cells, grown on 22 mm2 glass cover slips (VWR Scientific, Atlanta, GA, USA), were treated for 48 hours or 6 days with 5 ng/ml TGF-β1. After treatment, cells were washed once with phosphate buffered saline (PBS) and fixed with 100% cold methanol (for rat ZO-1 and E-cadherin antibody use), 4% paraformaldehyde/PBS (for F-actin staining), or 1% paraformaldehyde/PBS (for rabbit ZO-1 antibody use) for 20 min at 25°C. Cells were washed four times with PBS, permeabilized by incubation with 0.2% Triton X-100 (in PBS) for 10 min at 25°C, and then washed two more times with PBS. For ZO-1 and E-cadherin staining, nonspecific binding sites were blocked by cellular incubation for 2 hours with 5% serum (goat serum for rabbit ZO-1 and E-cadherin antibody use and rabbit serum for rat ZO-1 antibody use) in PBS, incubated in primary antibodies diluted in 5% serum/PBS (rat ZO-1 1:1000, rabbit ZO-1 1:100, and E-cadherin 1:2500) for 1 hour at 25°C, followed by four washes with PBS. Cells were incubated in appropriate biotinylated secondary antibodies diluted in 5% serum/PBS (1:250) for 1 hour at 25°C, washed four times with PBS, and incubated in streptavidin-conjugated Cy3 diluted in 5% serum/PBS (1:1000) for 1 hour at 25°C. Cells were washed four times with PBS and nuclei were counter-stained by incubation with 0.1 μg/ml Hoechst (33258) for 15 min at 25°C. For F-actin staining, cells were incubated in Texas Red-X phalloidin (Molecular Probes Inc., Eugene, OR, USA) diluted in PBS (1:200) for 30 min, washed with PBS three times, and were counterstained with Hoechst as described above.
After Hoechst staining, cells were washed three times with PBS and cover slips were mounted onto 25 × 75 mm microslides (Fisher Scientific, Pittsburgh, PA, USA) using AquaPolyMount (Polysciences, Warrington, PA, USA). Phase contrast images were captured using the Zeiss Epifluorescence inverted microscope and Zeiss AxioCam digital camera (Carl Zeiss, Jena, Germany). Fluorescent images were captured using the Zeiss Axiophot upright microscope (Carl Zeiss) and the Princeton Instruments cooled CCD digital camera (Princeton Scientific Instruments, Inc., Monmouth Junction, NJ, USA).
Transforming growth factor-β1 induced epithelial to mesenchymal transition in NMuMG and MCT cells
To determine the frequency of TGF-β1-mediated EMT in vitro, we performed a screen of 18 established cell lines from human and mouse epidermis, mammary gland, lung, pancreas, kidney, and prostate (Table 1). In addition to the established cell lines, primary cultures of human epidermal keratinocytes (HEKs) and human mammary gland epithelial cells (HMEC-1012 and HMEC-1016) were also screened (Table 1). In the present study, EMT was defined as acquisition of a spindle-shaped morphology, loss of ZO-1 and E-cadherin from cell–cell junctions, and formation of actin stress fibers after TGF-β1 treatment. Using phase contrast and immunofluorescence microscopy, we determined that only two cell lines underwent EMT. After 48 hours of TGF-β1 treatment, the NMuMG and MCT cells became elongated (Fig. 1a,1e,1i,1m), lost E-cadherin (Fig. 1b,1f,1j,1n) and ZO-1 (Fig. 1c,1g,1k,1o) staining at cell–cell junctions, and developed actin stress fibers (Fig. 1d,1h,1l,1p).
The primary cultures of breast epithelial cells (HMEC-1012 and HMEC-1016) acquired a spindle-shaped morphology, whereas the primary cultures of HEKs did not change cell morphology after 48 hours of TGF-β1 treatment (Fig. 2a,2e,2i,2m; and data not shown). In addition, the HMECs and HEKs developed actin stress fibers after treatment (Fig. 2d,2h,2l,2p; and data not shown). However, the HMECs and HEKs did not lose junctional E-cadherin staining (Fig. 2b,2f,2j,2n; and data not shown) after TGF-β1 treatment for 48 hours. These cells also had little or no ZO-1 localized to their cell–cell junctions (Fig. 2c,2g,2k,2o; and data not shown).
The human breast epithelial cell line MCF10A did not become elongated (Fig. 3a,3e) or lose junctional E-cadherin or ZO-1 staining (Fig. 3b,3f,3c,3g) in response to 48 hours of TGF-β1 treatment. After treatment, these cells exhibited some actin stress fiber formation (Fig. 3d,3h). However, the MCF10A cells acquired a spindle-shaped morphology (Fig. 3i,3m) and actin stress fibers (Fig. 3l,3p), and lost much of the junctional E-cadherin and ZO-1 (Fig. 3j,3n,3k,3o) after TGF-β1 treatment for 6 days. The HaCaT, UNC10, A549, Colo357, DU145, MK, KC, and 4T1 cells also exhibited an actin stress fiber response to TGF-β1, without delocalization of E-cadherin or ZO-1 from the cell–cell junctions, similar to the MCF10A cells after 48 hours of TGF-β1 treatment (Fig. 4b,4f,4r,4v,4c,4g,4s,4w,4d,4h,4t,4x; and data not shown).
Other cell lines screened did not exhibit any changes in cell morphology or relocalization of E-cadherin, ZO-1, or actin after treatment with TGF-β1. These cell lines included SCC012, SCC028, HBL100, BT549, MCF7, MDA-MB-231, MDA-MB-361, MDA-MB-435S, MDA-MB-436, MDA-MB-468, H1299, Panc-1, and EpH4 cells (Fig. 4i,4j,4k,4l,4m,4n,4o,4p; and data not shown). A summary of the TGF-β1-induced cellular response of the cell strains that exhibited acquisition of a spindle-shaped morphology, loss of junctional E-cadherin or ZO-1, or formation of actin stress fibers is presented in Table 2.
Transforming growth factor-β1-induced inhibition of S-phase
Previous studies analyzing TGF-β1 induction of EMT have emphasized the stages in which TGF-β1 acts as a promoter of carcinogenesis. It is proposed that cells first lose sensitivity to the growth inhibitory effects of TGF-β1, before TGF-β1 can promote EMT and cancer progression . Therefore, we examined whether there was a correlation between TGF-β1-mediated EMT and loss of sensitivity to the growth inhibitory effects of TGF-β1 by examining [3H]thymidine incorporation and flow cytometry.
In [3H]thymidine incorporation experiments, it was observed that 41% of the cell strains screened had a 0–25% reduction in [3H]thymidine incorporation (or 75% of the control) after 48 hours of TGF-β1 treatment. These cells included SCC028, UNC10, HBL100, MDA-MB-361, MDA-MB-435S, MDA-MB-436, MDA-MB-468, H1299, Colo357, Panc-1, and 4T1 (Fig. 5 and Table 3). Similarly, 37% of the cell strains screened had a 25–75% reduction in [3H]thymidine incorporation (or 75–25% of the control) after 48 hours of TGF-β1 treatment. These cells included HaCaT, SCC012, HMEC (1016), MCF10A, BT549, MCF7, MDA-MB-231, A549, DU145, and EpH4 (Fig. 5 and Table 3). Only 22% of the cell strains screened showed greater than a 75% reduction in [3H]thymidine incorporation (or 25% of the control) after 48 hours of TGF-β1 treatment (Fig. 5 and Table 3). These cells included HEK, HMEC (1012), MK, KC, NMuMG, and MCT (Fig. 5 and Table 3). Of note, established cell lines constituted 95% of the cells that did not have greater than 75% reduction in [3H]thymidine after TGF-β1 treatment (Fig. 5 and Table 3).
Most of the cell lines that did not have a greater than 75% reduction in [3H]thymidine incorporation after TGF-β1 treatment, did not exhibit changes in morphology or changes in actin, E-cadherin, or ZO-1 localization in this screen (Figs 1,2,3,4,5; and data not shown). Only the UNC10, A549, and DU145 cell lines did not have reduced [3H]thymidine incorporation of greater than 75% and had increased actin stress fiber formation after TGF-β1 treatment (Figs 4 and 5; and data not shown). However, there was no change in ZO-1 localization in these cells (data not shown). In comparison, all of the cell lines that had decreased [3H]thymidine incorporation had increased actin stress fiber formation after TGF-β1 treatment (Fig. 1d,1h,1l,1p; Fig. 2d,2h,2l,2p; Fig. 3d,3h,3I,3p; Fig. 4d,4h,4t,4x; Fig. 5; and data not shown). These cells included the HaCaT, MCF10A, Colo357, MK, KC, NMuMG, 4T1, and MCT cells, and the primary cultures of HMEC-1012 and HEK cells.
Flow cytometry was also performed on cells treated with TGF-β1 for 48 hours to confirm the data generated by [3H]thymidine incorporation. The data generated by flow cytometry experiments were consistent with those of [3H]thymidine incorporation (Figs 5 and 6, and Table 3). Fig. 6 includes histograms that were representative of cell strains with 0–25% (MDA-MB-436), 25–75% (EpH4), and 75–100% (NMuMG) reduction in S-phase after 48 hours of TGF-β1 treatment, when compared with the control cells.
Transforming growth factor-β1-mediated Smad2 phosphorylation did not correlate with S-phase reduction
To determine the relationship of Smad2 phosphorylation with reduction in S-phase and EMT, after TGF-β1 treatment, we analyzed phosphorylated Smad2 protein levels. Western analyses of protein extracts showed that, after 2 hours of treatment with TGF-β1, phosphorylated Smad2 protein levels increased in all of the cell strains screened except for the MCF7, MDA-MB-361, and MDA-MB-435S cells when normalized to actin (Fig. 7 and Table 3). After treatment with TGF-β1 for 48 hours, levels of phosphorylated Smad2 remained elevated in the cells with increased levels of phosphorylated Smad2 after 2 hours of treatment, except HMEC (1016), HBL100, MCF10A, MDA-MB-436, H1299, MK, and MCT when normalized to actin (Figs 7 and 8, and Table 3). Immunoblot analysis of the MCF7, MDA-MB-361, and MDA-MB-435S cells with the phosphorylated Smad2 antibody (lot #21034) resulted in a band (indicated by an asterisk) that migrated higher than the phosphorylated Smad2 protein (Fig. 7).
Cell strains that exhibited TGF-β1-induced phosphorylation of Smad2 did not necessarily exhibit a reduction in [3H]thymidine uptake. These cell strains included SCC028, MDA-MB-436, MDA-MB-468, and H1299 (Figs 5 and 7, and Table 3). Although the MCF7 cells had [3H]thymidine uptake of 59% of the control after 48 hours of TGF-β1 treatment, an increase in phosphorylation of Smad2 by Western analysis was not observed at 2 hours or at 48 hours (Figs 5, 7 and 8, and Table 3).
Prolonged transforming growth factor-β1 treatment led to decreased total Smad2 and Smad3 protein levels in many cell strains
Total Smad2 and Smad3 protein levels decreased with TGF-β1 treatment in 51% and 48% of the cell lines, respectively (Fig. 8). Total Smad2 levels decreased in HEK, HaCaT, SCC012, UNC10, BT549, MDA-MB-231, MDA-MB-361, MDA-MB-435S, H1299, Colo357, NMuMG, EpH4, 4T1, and MCT cells when normalized to actin (Fig. 8). Total Smad3 levels decreased in HEK, HMEC (1012 and 1016), HaCaT, SCC012, SCC028, UNC10, BT549, MDA-MB-231, MDA-MB-436, A549, EpH4, and 4T1 cells when normalized to actin (Fig. 8).
Decreased total Smad2 and total Smad3 protein levels did not correlate with an increased reduction in S-phase after TGF-β1 treatment for 48 hours. For instance, the HMEC (1012), MK, and KC cells had a 87%, 81%, and 89% reduction in [3H]thymidine incorporation, respectively, whereas there was no decrease in total Smad2 protein levels after 48 hours of TGF-β1 treatment (Figs 5 and 8, and Table 3). Similarly, the MK, KC, MCT, and NMuMG cells had 81%, 89%, 76%, and 92% reductions in [3H]thymidine incorporation, respectively, whereas there was no decrease in total Smad3 protein levels after 48 hours of TGF-β1 treatment (Figs 5 and 8, and Table 3). In contrast, the HEK cells had a 98% reduction in [3H]thymidine incorporation and had no reduction of total Smad2 or Smad3 after 48 hours of TGF-β1 treatment (Figs 5 and 8, and Table 3).
Also, decreased total Smad2 and Smad3 protein levels did not correlate with an increase in the levels of phosphory-lated Smad2 protein after TGF-β1 treatment (Figs 7 and 8, and Table 3). An increase in phosphorylated Smad2 protein levels occurred in all cell strains screened after 2 hours of TGF-β1 treatment except for the MCF7, MDA-MB-361, and MDA-MB-435S cells (Fig. 7), whereas only a subset of those had decreased total Smad2 and/or Smad3 protein levels after TGF-β1 treatment for 48 hours (Fig. 8 and Table 3). Additionally, the MDA-MB-361 and the MDA-MB-435S cells did not have increased phosphorylated Smad2 levels or decreased total Smad3 levels, but they did exhibit decreased total Smad2 levels after 48 hours of TGF-β1 treatment (Figs 7 and 8, and Table 3).
The decrease in total Smad2 and Smad3 protein levels, observed after TGF-β1 treatment, did not associate with the ability of the cell line to undergo TGF-β1-mediated EMT. NMuMG and MCT cells underwent EMT (Fig. 1) and they both exhibited decreased total Smad2 and no decrease in total Smad3 protein levels after TGF-β1 treatment for 48 hours (Fig. 8). The other cell lines that had decreased total Smad2 and no decrease in total Smad3 levels after TGF-β1 treatment did not undergo TGF-β1-induced EMT (Figs 2,3,4 and 8, and Table 3; and data not shown).
TGF-β1 is an inhibitor of epithelial cell growth in the early stages of carcinogenesis. However, it also promotes tumor cell invasion and metastasis through the induction of EMT . Many studies on the mechanism of TGF-β1-induced EMT are limited to a few murine cell lines and mouse models. Therefore, to identify alternative cell systems in which to study TGF-β1-induced EMT, we performed a TGF-β1 sensitivity screen using a panel of human primary cells and established human and mouse cell lines.
The TGF-β1-induced morphologic changes observed in the NMuMG, MCT, and HMEC cells 48 hours after TGF-β1 treatment are consistent with changes seen during EMT (Fig. 1a,1e,1i,1m; Fig. 2i,2m; and data not shown) [53, 54]. Changes in cell morphology, from a cobblestone-like appearance to more elongated shape, and actin stress fiber formation, were observed in the NMuMG and MCT cells, and in primary cultures of HMECs (Fig. 1a,1d,1e,1h,1i,1l,1m,1p; Fig. 2i,2l,2m,2p; and data not shown). However, only the NMuMG and MCT cells lost E-cadherin and ZO-1 staining at the cell-cell junctions after 48 hours of TGF-β1 treatment (Fig. 1b,1f,1j,1n,1c,1g,1k,1o). E-cadherin is a protein found at adherens junctions that allows for cell–cell adherence, and ZO-1 is a tight junctional protein that forms a selective barrier between cells. Loss of these proteins at cell–cell junctions is used as a marker of EMT [54, 60–63]. Cortical actin is a measure of cell integrity and loss thereof, or formation of actin stress fibers, is also used to define EMT [63, 64]. Therefore, we concluded that only the NMuMG and MCT cells underwent TGF-β1-mediated EMT, after 48 hours of treatment, in this screen. Results from previous studies also show that NMuMG and MCT cells undergo TGF-β1-mediated EMT [60, 61, 63–65]. Other studies reported that TGF-β1-mediated EMT occurs in HaCaT, Colo357, and Panc-1 cells 48 hours after TGF-β1 treatment [66, 67]; however, they did not undergo TGF-β1-induced EMT according to the conditions used in the present study (Fig. 4). Other cell lines screened in the study formed actin stress fibers with TGF-β1 treatment, but they did not lose ZO-1 from cell–cell junctions (Fig. 3c,3d,3g,3h; and data not shown). We did not examine E-cadherin localization in all of the cell strains because not all of the cell strains exhibited morphologic changes, with TGF-β1 treatment, that were indicative of EMT.
Unlike the mouse NMuMG and MCT cells, none of the 14 human cell lines with an epithelial morphology screened underwent TGF-β1-mediated EMT within 48 hours of TGF-β1 treatment. The MCF10A human breast epithelial cell line took 6 days to undergo a morphologic change, lose junctional E-cadherin and ZO-1, and form actin stress fibers with TGF-β1 treatment (Fig. 3i,3j,3k,3l,3m,3n,3o,3p). However, this extended treatment with TGF-β1 to induce EMT is not consistent with previous reports that used times up to and including 48 hours [60, 61, 66, 67]. It may be that the extended treatment with TGF-β1 is necessary to activate secondary and tertiary signaling pathways that are not activated within 48 hours. The Panc-1, Colo357, and HaCaT cells were treated with TGF-β1 for longer than 48 hours because they were shown to undergo TGF-β1-induced EMT in previous reports [66, 67]. However, these cell lines did not undergo EMT when treated with TGF-β1 for 72 hours (data not shown). These data could suggest that human cells are more resistant to TGF-β1-mediated EMT. Alternatively, the TGF-β1 treatment times were not long enough to induce EMT, the small sample size used may not be representative, or the cells may not have the genetic alterations necessary for TGF-β1 to induce EMT.
Activation of non-Smad signaling pathways is also implicated in TGF-β1-mediated EMT. Many studies have shown a requirement for activated Ras/Raf/mitogen-activited protein kinase for TGF-β1-mediated EMT in human, rat, or mouse epidermal, pancreas, intestine, liver, prostate, and mammary epithelial cells [67–76]. In the mouse mammary gland epithelial cell line EpH4, TGF-β1 induces EMT and tumor formation in mice only when cells express oncogenic H-Ras . Furthermore, it has been shown that TGF-β1 can activate Ras, and increased H-Ras levels are required for nuclear accumulation of Smad2 . Additionally, signaling through integrin β1  and activation of EGF receptor , RhoA , p38 mitogen-activited protein kinase , and phosphatidylinositol 3-kinase [60, 70, 71] pathways are involved in or required for TGF-β1-induced EMT.
The lack of TGF-β1-mediated EMT in the human cells does not necessarily refute a role for TGF-β1 in promoting EMT in vivo in human tumors. Human epithelial tumors can undergo mesenchymal conversions, providing a potential role for EMT in human metastasis. It has been shown that excess TGF-β1 can promote EMT in human tumors in vivo. Increased levels of TGF-β1 are observed in many human tumors [35–40, 42, 51, 78–80], are often localized to the advancing edges of primary tumors and metastases, and are associated with poor clinical outcome [39, 41].
It is somewhat unexpected that TGF-β1-induced EMT occurred in nontransformed cell lines, such as the NMuMG and MCT cells, because in vivo mouse studies show that TGF-β1 promotes tumor cell invasion and metastasis in the later stages of carcinogenesis [5, 6]. In one of these studies, targeted expression of TGF-β1 to mouse suprabasal keratinocytes results in resistance to the formation of benign skin tumors, after long-term chemical carcinogenesis treatment. However, benign papillomas that develop become malignant at an accelerated rate and metastasis occur more rapidly than spontaneous tumors in control mice. Additionally, there are a high incidence of spindle cell carcinoma development in these mice, pointing to TGF-β1-induction of EMT in vivo . NMuMG and MCT cells may have the genetic alterations that allow for TGF-β1-mediated EMT to occur.
Many studies on TGF-β1-mediated EMT have emphasized that TGF-β1 promotes carcinogenesis in stages. It is proposed that cells first lose sensitivity to the growth inhibitory effects of TGF-β1, and subsequently TGF-β1 can promote tumor progression and EMT . MMH-D3 murine hepatocytes and EpH4 murine mammary gland epithelial cells undergo TGF-β1-mediated EMT only when rendered insensitive to TGF-β1-induced cell cycle arrest or apoptosis, by infection with active H-Ras [59, 70, 73, 81]. However, the present study does not support this model because it shows that resistance to the growth inhibitory effects of TGF-β1 is not a prerequisite for TGF-β1-mediated EMT. The NMuMG and MCT cells exhibited a decrease in S-phase and underwent EMT after 48 hours of TGF-β1 treatment (Figs 1, 5, and 6). Consistent with the present study were experiments performed by Nicolas and coworkers  that showed that increased Smad3 in MDCK cells restored growth inhibitory responses to TGF-β1 but did not revert cells from a mesenchymal to an epithelial phenotype. Additionally, Chang and coworkers  observed that increased TGF-β1 expression in sarcoma cells increased cell tumori-genicity while inhibiting cell proliferation.
The trends observed with the analysis of the flow cytometry data were consistent with the [3H]thymidine incorporation data (Figs 5 and 6 and Table 3). However, the values for the percentage of the control cells in S-phase were not identical between [3H]thymidine incorporation and flow cytometry for each cell strain. This discrepancy can be accounted for by the fact that the data were generated using two different methodologies. [3H]thymidine incorporation examines DNA synthesis during the last 2 hours of the 48-hour period, whereas flow cytometry examines DNA synthesis at the 48-hour time-point. Although the numeric data generated from the [3H]thymidine incorporation and flow cytometry experiments were not the same, the trends of TGF-β1-induced decreases in DNA synthesis were consistent.
All but three of the cell strains screened had an increase in phosphorylated Smad2 protein levels after 2 hours of TGF-β1 treatment, but not all of the cell lines that had increased phosphorylation of Smad2 had reduced S-phase after 48 hours of TGF-β1 treatment. The SCC028, MDA-MB-436, MDA-MB-468, and H1299 cells had an increase in phosphorylated Smad2 levels after 2 hours of TGF-β1 treatment, but they exhibited decreases in S-phase of only 5%, 1%, 4%, and 4%, respectively (Figs 5,6,7 and Table 3). The lack of S-phase decrease upon 48 hours of TGF-β1 treatment may point to inactivation of or mutations in downstream proteins that could abolish TGF-β1-mediated growth inhibition in these cells. The MCF7 cells did not exhibit an increase in phosphorylated Smad2 protein levels after 2 hours of TGF-β1 treatment, but there was a 41% decrease in S-phase on 48 hours of TGF-β1 treatment (Figs 5,6,7, and Table 3). This decrease in S-phase is not as great a decrease as was exhibited by some of the other cell strains when treated with TGF-β1 for 48 hours. The decrease could be explained by very low levels of phosphorylated Smad2 increase on TGF-β1 treatment that was not detected by immunoblot analysis. Alternatively, it is possible that the TGF-β1 signal was propagated by phosphorylation of Smad3.
Smad2 is not solely responsible for the propagation of TGF-β1 signals. Similar to Smad2, on TGF-β1 binding to the TβRII, Smad3 is phosphorylated by the TβRI, forms a complex with Smad4, translocates to nucleus, and regulates the activation of TGF-β1 target genes. However, mutations or deletions in Smad3 are rare in human cancers. Reports by Graham and coworkers  and Xu and coworkers  suggest that loss of Smad3 may largely be responsible for the nonresponsiveness of some cells to TGF-β1. The proliferation, migration, and invasion of normal extravillous trophoblast cells are under the control of TGF-β1. However, premalignant and malignant trophoblast cells, that have lost the Smad3 protein but retain functional Smad2, are resistant to the antiproliferative and anti-invasive effect of TGF-β1. It is therefore possible that the attenuation of inhibition of S-phase or the induction of EMT by TGF-β1 in the present study may be a result of mutation or loss of Smad3, even though the cells have increased phosphorylation of Smad2 on TGF-β1 treatment.
Interestingly, decreased total Smad2 and Smad3 protein levels were observed after TGF-β1 treatment regardless of changes in the levels of phosphorylated Smad2 protein or of whether cell proliferation was inhibited by TGF-β1 (Figs 5,6,7,8). Similar to our findings, decreased total Smad2 protein levels were reported in COS-1 monkey kidney cells after TGF-β1 treatment . In that report, the proteasome inhibitors MG-132 or lactacystin blocked Smad2 from TGF-β1-induced degradation. In addition, Smad3 decreases have been reported during TGF-β1-induced EMT in MDCK cells [72, 85] and after TGF-β1 treatment of human lung epithelial cells . In these studies, MDCK cells become refractory to the growth inhibitory effects of TGF-β1 [72, 85]. TGF-β1 treatment of primary human fibroblasts and HaCaT cells also leads to decreased total Smad3 protein levels [87, 88].
A negative feedback loop could explain the decreases in total Smad2 and Smad3 protein levels after 48 hours of TGF-β1 treatment. The E3 ubiquitin ligase Smurf has been shown to interact with Smads and promote their ubiquitination [89, 90]. In this model, phosphorylated, nuclear Smad2 is ubiquitinated by Smurf2 and degraded by proteasomes [89, 90]. Smad7 also interacts with Smurf2 and induces TGF-β receptor degradation [91, 92]. Phosphorylated Smad3 is also ubiquitinated by the ROC1-SCFFbw1aE3 ligase complex, and subsequently degraded in the proteasome . In order to prevent continuous Smad signaling in the absence of TGF-β1 stimulation, Smad2 and Smad3 are negatively regulated by a number of proteins. Smad6 and Smad7 inhibit Smad2 and Smad3 activation by competing with Smad2 and Smad3 for binding to the TGF-β receptors . Smad6 and Smad7 are induced by activation of TGF-β1 signaling and form a negative feedback loop [94–96]. However, the mechanism of decrease in total Smad2 and/or Smad3 in different cell strains on prolonged TGF-β1 treatment remains unclear.
TGF-β1 induction of EMT is a rare occurrence in vitro and is not limited to transformed cell lines. In fact, TGF-β1-mediated EMT was only observed in nontumorigenic cells in the present study. Furthermore, there does not appear to be a correlation between loss of TGF-β-mediated growth inhibition and EMT. The inability of TGF-β1 to induce EMT was not due to a total loss of TGF-β1 signaling, as was evidenced by induction of Smad2 phosphorylation. In conclusion, our data indicate that the in vitro models used to study TGF-β1 induction of EMT may not be as relevant to in vivo cancer progression as was previously assumed in the field.
Dulbecco's modified Eagle's medium
epidermal growth factor
epithelial to mesenchymal transition
fetal bovine serum
human epidermal keratinocytes
human mammary epithelial cell
mouse keratinocytes transformed with K-ras
minimal essential medium
phosphate buffered saline
Sma/Mothers Against Decapentaplegic
TGF-β type I receptor
TGF-β type II receptor
transforming growth factor
Tris buffered saline with Tween-20
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We thank the Vanderbilt University Toxicology Center tissue culture core facility (supported by NIH grant ES00267) and the Vanderbilt University Medical Center Cell Imaging Core Resource (supported by NIH grants CA68485 and DK20593). We would also like to thank Dr Brian Law, Dr Neil Bhowmick, Dr Matthew Westfall, Jamie Hearnes, and Kristy Schavolt for critical reading of the manuscript. The present study was also supported by NIH training grant T32CA09592 to KAB and R01 CA85492 and R01 CA102162 to HLM.
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Brown, K.A., Aakre, M.E., Gorska, A.E. et al. Induction by transforming growth factor-β1 of epithelial to mesenchymal transition is a rare event in vitro . Breast Cancer Res 6, R215 (2004). https://doi.org/10.1186/bcr778
- epithelial to mesenchymal transition