Abstract
Transforming growth factor-β1 (TGF-β1) is involved in tumor progression by promoting angiogenesis or suppressing the immune system; yet TGF-β1 also has a growth-inhibitory effect on epithelial cells including carcinoma cells. Several mechanisms of impaired TGF-β1 responsiveness of carcinoma cells have been reported. In this study, we examined how TGF-β1 participates in the development and progression of intrahepatic cholangiocarcinoma (ICC) associated with hepatolithiasis, and how ICC cells escape from growth inhibitory effect of TGF-β1. A total of 40 cases of hepatolithiasis were studied, including 16 cases of ICC, and in vitro studies were conducted with cultured murine non-neoplastic biliary epithelial cells (MBEC) and three ICC cell lines. Immunohistochemically, TGF-β1 was expressed in mononuclear cells and mesenchymal cells around the stone-containing bile ducts and invasive ICC, and also in biliary epithelial cells (hyperplastic and precursor lesions, and ICC). TGF-β type II receptor (TβR-II) was constantly expressed on biliary epithelial cells irrespective of biliary lesions. In cell culture studies, TGF-β1 significantly inhibited proliferation of MBEC via downregulation of cyclin D1, cdk4, and cdk6, while TGF-β1 did not influence the proliferation of ICC cells. After suppression of cyclin D1 expression in one ICC cell line using cyclin D1 small interfering RNA, TGF-β1 significantly inhibited the proliferation of ICC cells. In conclusion, high levels of TGF-β1 around ICC or its precursors may be involved in development and progression of ICC in hepatolithiasis. ICC cells could escape the growth inhibitory effect of TGF-β1 by overexpression of cyclin D1.
Similar content being viewed by others
Main
Three isoforms of transforming growth factor-β (TGF-β) (TGF-β1, -β2, -β3) have been identified in humans, and they have similar biological functions.1, 2 TGF-β signal is transducted through two surface receptors, the TGF-β type I receptor (TβR-I) and the TGF-β type II receptor (TβR-II), that function as a complex. TβR-I and TβR-II possess intracellular serine/threonine kinase domains that are activated upon complex formation.3 This kinase in turn initiates an intracellular signal cascade to the nucleus by activation of various proteins, including Smad.4, 5
Among the TGF-βs, TGF-β1 has been extensively studied with respect to its involvement in the carcinogenic process. TGF-β1 has several advantageous effects for carcinoma cells such as modulating fibrogenesis, angiogenesis, and immune modulation.4, 6 Overexpression of TGF-β1 has been reported in some carcinomas, and is thought to be involved in carcinogenesis and tumor progression.6, 7 Moreover, overexpression of TGF-β1 in carcinoma cells is also known as an influential prognostic factor in breast cancer and lung cancer patients.8, 9
While TGF-β1 has growth inhibitory effects on non-neoplastic epithelial cells, proliferation of most carcinoma cells is not influenced by TGF-β1.1, 10 This is also the case with cholangiocarcinoma cells. For example, Yokomuro et al11 reported that TGF-β1 exerted a concentration-dependent mito-inhibition effect on non-neoplastic biliary epithelium, whereas cholangiocarcinoma cells were resistant to TGF-β1. Carcinoma cells are thought to gain resistance to the growth inhibitory effects of TGF-β1 by several mechanisms. Somatic mutations of TβR-II were firstly reported in some carcinoma cells, especially hereditary nonpolyposis colorectal cancer,12, 13 though the frequency was found to be relatively low in other carcinomas.14, 15 Other mechanisms of escaping tumor growth inhibition by TGF-β1 such as somatic mutation of Smads, transcriptional downregulation of TGF-β receptors, and overexpression of smad7, are also reported.16, 17, 18, 19
TGF-β1 is known to inhibit the proliferation of non-neoplastic epithelium at the G1/S phase via several cell cycle-related molecules such as cyclins (cyclins D, cyclin E), cdks (cdk2, cdk4, cdk6), and cdk inhibitors (p15, p21, p27).20, 21, 22, 23 TGF-β1 executes its growth-inhibitory effect by downregulation of mito-activators (cyclins and cdks) and by upregulation of mito-inhibitors (p15, p21, p27), although the pattern and degree of these effects are different depending on the cell type. Disorganized expression of those cell cycle-related molecules could also induce TGF-β1-resistance in some neoplastic cells.24 For example, TGF-β1 is reported to downregulate expression of cyclin D1, one of the necessary molecules for the transition from the G1 to the S phase of the cell cycle, in non-neoplastic epithelial cells such as rat intestinal epithelial cells.20, 23 In neoplastic cells, overexpression of cyclin D1 could induce their unresponsiveness to growth inhibitory effect of TGF-β1.25, 26 These data suggest that cyclin D1 is thought to be one of the key molecules involved in TGF-β-unresponsiveness of some carcinoma cells.
In this study, we examined the participation of TGF-β1 and TβR-II in the development of ICC in hepatolithiasis by immunohistochemistry, by examination of genetic mutations in exons 3, 5, and 7 of the TβR-II gene by polymerase chain reaction-single strand conformation polymorphism (PCR-SSCP), and by examination of the relationship between overexpression of cyclin D1 and responsiveness to TGF-β1 in cultured cells.
Materials and methods
Human Tissue Studies
Patients and materials
A total of 40 cases of surgically resected hepatolithiasis were obtained from the liver disease file of the Department of Human Pathology, Kanazawa University Graduate School of Medicine, and that of the Department of Pathology, Chang Gung Memorial Hospital, Lin Kou (Table 1). In all, 16 of these cases were associated with ICC (see below). In addition, ‘histologically normal’ liver tissues were obtained from non-neoplastic parts of five surgically resected metastatic liver tumors.
All of these specimens were fixed in formalin, and embedded in paraffin. All hepatolithiasis cases and five normal liver tissue were used for the immunohistochemistry, and 16 ICC cases were examined for mutational analysis of the TβR-II gene.
Classification of biliary lesions associated with hepatolithiasis
Biliary epithelial lesions of hepatolithiasis were classified into five categories (Table 1): biliary hyperplasia, biliary dysplasia, intraductal papillary neoplasm of the bile duct (IPN-B), ICC with dysplasia, and ICC with IPN-B. All of these biliary lesions were found in the stone-containing intrahepatic large bile ducts, which correspond to the first to third branches of the right and left hepatic ducts.27 Biliary dysplasia was defined as flat or micropapillary proliferation of epithelial cells showing multilayering, piled-up nuclei, an increased nucleocytoplasmic ratio, a partial loss of nuclear polarity, and nuclear hyperchromasia and pleomorphism.28 IPN-B was defined as prominent papillary proliferation of biliary epithelial cells with distinct fibrovascular cores, showing epithelial nuclear stratification, piled-up nuclei, and nuclear enlargement.29 ICC cases were classified into two groups: ICC with dysplasia (nine cases) and ICC with IPN-B (seven cases), in which biliary dysplasia and IPN-B were observed in bile ducts around ICC lesions (invasive lesions), respectively. ICC with dysplasia was histologically composed of well differentiated (one case), moderately differentiated (six cases), and poorly differentiated adenocarcinoma (two cases), while ICC with IPN-B showed well differentiated papillary adenocarcinoma (two cases), and mucinous carcinoma (five cases).
Immunohistochemistry
Deparaffinized sections 3?μm thick for TGF-β1 and TβR-II were first treated with hyaluronidase (2?mg/ml, Sigma Chemical Co., St Louis, MO, USA) for 2?h at 37°C. Sections for cyclin D1 were microwaved in EDTA buffer (pH 8.0) for 20?min. After blocking of endogenous peroxidase, the sections were incubated in Protein Block Serum (Dako, Glostrup, Denmark) for 20?min, then incubated overnight at 4°C with either of primary antibodies: anti-human TGF-β1 (clone 9016.2, 5?μg/ml, mouse monoclonal, R&D Systems, Minneapolis, MN, USA), anti-human TβR-II (2?μg/ml, gout polyclonal, R&D Systems), and anti-human cyclin D1 (clone AY-7D2, prediluted, mouse monoclonal, ZYMED Laboratories, San Francisco, CA, USA). These sections were incubated for 1?h with goat anti-mouse immunoglobulins (TGF-β1 and cyclin D1), or rabbit anti-goat immunoglobulins (TβR-II), both of which were conjugated to peroxidase labeled polymer (Envision+, Dako; Histofine Simple Stain MAX PO(G), Nichirei, Tokyo, Japan). After 3,3′-diaminobenzidine tetrahydrochloride (DAB) reaction, the sections were lightly counterstained with hematoxylin (TGF-β1 and TβR-II) or methyl green (cyclin D1). Negative controls were evaluated by nonimmunized mouse or goat serum for primary antibody.
Evaluation of immunohistochemistry
Expression of TGF-β1 and TβR-II in individual biliary lesions was evaluated as positive or negative. Expression of cyclin D1 was evaluated by percent of positive cells counted in more than 1000 cells chosen at random in individual case (cyclin D1 labeling index). The labeling index was compared among the biliary lesions.
Mutation screening of the TβR-II gene with PCR-SSCP
Genomic DNA of ICC (16 cases) was extracted from paraffin tissue using DEXPAD (Takara, Tokyo, Japan). Serial 2-μm paraffin sections of ICC (invasive lesions) were microscopically dissected and mixed with DAXPAD (Takara) at 100°C for 10?min. DNA similarly extracted from nontumorous areas of ICC was used as a wild type (nonmutated) control. DNA was obtained by centrifugation and used as a template for PCR.
Three sets of primers were designed to amplify the entire exon sequences for 3, 5, and 7 of the TβR-II gene, including each splicing site, as follows: exon 3, sense 5′-cctcgcttccaatgaatctc-3′, antisense, 5′-ttggcacagatctcaggtcc-3′; exon 5, sense 5′-aatgatggcctcactgtctg-3′, antisense 5′-ccactacacatatctggtcc-3′; exon 7, sense 5′-cctttggatctctttcccgc-3′, antisense 5′-agaggggcagcctctttgg-3′. PCR consisted of 40 cycles at 94°C for 1?min, at 50°C for 2?min, and at 72°C for 2?min. Product sizes of exon 3, 5, and 7 were 267, 202 and 249?bp, respectively. PCR products were subjected to electrophoresis carried out on acrylamide gels (GeneGel Excel 12.5/24 Kit, Amersham Pharmacia Biotech, Uppsala, Sweden) on GenePhor (Amersham Pharmacia Biotech). The running conditions were 300?V at 15°C for 2?h, and the gels were stained with silver (DNA Silver Staining Kit, Amersham Pharmacia Biotech).
Cell Culture Studies
Cell culture
Three human ICC cells (CCKS1, HuCCT1, and HuH28) were used in this study. CCKS1.30, 31 was established in our laboratory, and HuCCT132 and HuH2833 were obtained from the Health Science Research Resources Bank (Osaka, Japan). The murine-derived non-neoplastic biliary epithelial cell line (MBEC) was used as control (non-neoplastic biliary epithelial cells), established in our laboratory from intrahepatic large bile duct of an 8-week-old female BALB/c mouse.34 A mouse non-noeplastic cell line was used because human-derived non-neoplastic biliary epithelial cells from intrahepatic large bile ducts are difficult to purify and culture with continuous passages.
ICC cells were cultured with medium composed of D-MEM/F-12 (Dulbecco's modified Eagle medium and nutrient mixture F-12, 1:1; Life Technologies, Inc., Rockville, MD, USA), 10% fetal bovine serum (FBS) (Life Technologies, Inc.), and 1% antibiotics-antimycotic (Life Technologies, Inc.). MBEC were cultured on a collagen-coated dish, and were incubated with a culture medium composed of D-MDM/F-12 (Life Technologies, Inc.), 10% Nu-Serum (Becton Dickinson Labware, Bedford, MA, USA), 1% ITS+ (Becton Dickinson Labware), 5?μ M Forskolin (Wako Pure Chemical Industries, Ltd., Osaka, Japan), 12.5?mg/ml of Bovine pituitary extract (Life Technologies, Inc.), 1?μ M dexamethasone (Sigma Chemical Co., St Louis, MO, USA), 5?μM triiodo-thyronine (Sigma Chemical Co.), 5?mg/ml of Glucose (Sigma Chemical Co.), 25?mM Sodium bicarbonate (Sigma Chemical Co.), 1% antibiotics–antimycotic (Life Technologies, Inc.) and 25?ng/ml of mouse epidermal growth factor (Life Technologies, Inc.). These cells were cultured for cell proliferation assay in 96-well plates and also cultured for protein extraction in 60?mm culture vessels.
Influence of TGF-β1 treatment on cell proliferative activities and expression of cell cycle related molecules
ICC cells (CCKS1, HuCCT1, HuH28) and MBEC for proliferation assay were cultured with human TGF-β1 (Genzyme/Techne, Cambridge, MA, USA) and recombinant TGF-β1 (R&D systems, Inc.) at the concentration of 0.3, 3.0, and 30.0?ng/ml for 48?h, respectively. Recombinant TGF-β1 used in this study was reported to function on murine-derived cell lines.35 TGF-β1 treatment on cell proliferation study of HuH28 was started at about 50% cell-density, because HuH28 had low-proliferative activity (doubling time: 7 days).
Cells for RT-PCR and Western blot analysis were incubated with TGF-β1 at a concentration of 3.0?ng/ml for 48?h. The concentration of 3.0?ng/ml was determined based on our preliminary research and previous reports.20, 21
Cell proliferation assay
Cell proliferation was assayed by CellTiter 96 Aqueous One Solution Cell Proliferation (Promega, Madison, WI, USA). Briefly, 100?μl of the cell suspension (containing 1.0 × 104. cells) was plated in each well of 96-well plates. After confirming reattachment of cultured cells, some group of cells were transfected, and were followed by incubation with basic medium or TGF-β1 containing medium for 48?h. A amount of 20?μl of the CellTiter 96 Aqueous One Solution Reagent was added to each well. After incubation for 3?h, 490?nm absorbance was measured. Five samples for each group were used for analysis.
Western blot
Proteins were extracted from cultured cells using T-PER™ Tissue Protein Extraction Reagent (Pierce Chemical Company, Rockford, IL, USA), and were used for Western blot analysis. Western blot analysis was carried out on 10% SDS-PAGE gel. The proteins in the gel were electrophoretically transferred onto nitrocellulose membrane. The membranes were incubated with primary antibodies to cyclin D1 (clone HD11, 1:100, mouse monoclonal, Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA), cyclin D2 (clone M-20, 1:100, rabbit polyclonal, Santa Cruz Biotechnology, Inc.), cyclin D3 (clone D-7, 1:100, mouse monoclonal, Santa Cruz Biotechnology, Inc.), cdk2 (clone H-298, 1:200, rabbit polyclonal, Santa Cruz Biotechnology, Inc.), cdk4 (clone H-303, 1:200, rabbit polyclonal, Santa Cruz Biotechnology, Inc.), cdk6 (clone H-96, 1:200, rabbit polyclonal, Santa Cruz Biotechnology, Inc.), TβR-II (2?μg/ml, goat polyclonal, R&D Systems, Inc.), or β-actin (clone AC-15, 1:5000, mouse polyclonal, Abcam Limited, Cambridge, UK). All of these antibodies were designated for both human and murine research.
Each protein expression was detected using second antibodies conjugated to peroxidase labeled polymers such as Histofine Simple Stain MAX PO (G) (Nichirei) for TβR-II and EnVision+ system (Dako) for cyclin D1, cyclin D2, cyclin D3, cdk2, cdk4, cdk6, and β-actin. DAB was used as the chromogen.
Transfection of cyclin D1 small interfering RNA
HuH28, which is a less passaged strain, was selected for small interfering RNA (siRNA) transfection because highly passaged cells are not suited for siRNA transfection. A 21-nucleotide double-stranded RNA was synthesized by B-Bridge International Inc. (San Jose, CA, USA). The targeting sequence of human cyclin D1 was 5′-aagaugaaggagaccaucccc-3′, corresponding to the coding region 334–356 relative to the first nucleotide of the start codon. Scramble siRNA was used as a negative control, which targets the sequence 5′-gcgcgcuuuguaggauucg-3′. The siRNA were transfected to HuH28 cells with LipofectAMINE PLUS (Invitrogen Corp., Carlsbad, CA, USA). Of 20?μ M siRNA, 20?μl was diluted with 500?μl of OPTI-MEM I (Life Technologies, Inc.). An amount of 15?μl of PLUS reagent was added to the siRNA, and incubated for 15?min at room temperature. A volume of 25?μl of LipofectAMINE reagent was diluted with 500?μl of OPTI-MEM I. The two mixtures above were combined, gently mixed, and incubated for 15?min at room temperature. The entire mixture was added to the 4?ml of culture medium with cells in 6?mm vessels. A measure of 20?μl of this mixture was also added to 100?μl of the medium with cells in 96-well plates. At 24?h after transfection, some groups of cells were treated with TGF-β1 as mentioned above. At 72?h after transfection, the cells were used for the proliferation assay and protein extraction.
Statistical Analysis
The Mann–Whitney's U-test was employed with a significance level of P<0.05.
Results
Human Tissue Studies
Immunohistochemical detection of TGF-β1, TβR-II and cyclin D1
TGF-β1 expression was always detected in the cytoplasm of many inflammatory mononuclear and mesenchymal cells around the intrahepatic large bile duct in hepatolithiasis irrespective of epithelial lesion (Figure 1). TGF-β1 expression was also detected in those around invasive ICC. TGF-β1 was expressed as a diffuse and granular cytoplasmic staining pattern in hyperplastic biliary epithelium (70%), dysplastic epithelium (100%), IPN-B (100%), and ICC with dysplasia (89%) or IPN-B (86%), and a majority of these epithelial cells were positive, when detected (Figure 2a–c, and Table 2). However, its expression was not observed in normal bile ducts. TβR-II was constantly expressed in normal, hyperplastic, dysplastic, and neoplastic (IPN-B and ICC) biliary epithelium in all the cases (Figure 2d–f, and Table 2).
Cyclin D1 was expressed in the nuclei of all cases of biliary dysplasia (range: 4–15%), IPN-B (2–20%), ICC with dysplasia (5–60%) and ICC with IPN-B (5–55%) (Figure 3), but not expressed in normal bile ducts or biliary hyperplasia (Table 3). The labeling index of cyclin D1 was higher in ICC with dysplasia or IPN-B than in biliary dysplasia or IPN-B (P<0.05).
Mutation analysis of the TβR-II gene in ICC
Mutations of the TβR-II gene in exon 3, 5, and 7, in which most mutations of TβR-II genes are reportedly located, were examined by PCR-SSCP. PCR products included the splicing sites, so all sequences of each exon could be examined and evaluated. The results of SSCP analysis are shown in Figure 4. No shifted bands were observed in the exons of any cases examined or in the no-mutation control (WT), suggesting no genetic mutation existed in the three exons of the 16 ICC cases examined.
Cell Culture Studies
Influence of TGF-β1 on proliferative activities of cultured cells
As shown in Figure 5, TGF-β1 treatment showed inhibition on proliferation of MBEC, when compared to those without treatment. Treatment with 3.0 and 30.0?ng/ml of TGF-β1 more significantly inhibited the proliferation of MBEC compared to treatment with 0.3?ng/ml of TGF-β1. In contrast, proliferative activities of three cultured ICC cell lines were higher than MBEC, and were not influenced by the treatment of TGF-β1 compared to those without treatment. The amount of TGF-β1 (0.3, 3.0, and 30.0?ng/ml) did not influence on the proliferative activities of three ICC cells.
Expression of cell cycle-related molecules in cultured cells by TGF-β1 treatment
Western blot analysis of cyclin D1, cyclin D2, cyclin D3, cdk2, cdk4, and cdk6 after treatment of TGF-β1 disclosed that the level of cyclin D1 expression was evidently different between MBEC and ICC cells (CCKS1, HuCCT1, and HuH28) (Figure 6). That is, TGF-β1 treatment completely inhibited cyclin D1 expression in MBEC, but did not influence cyclin D1 expression in any of ICC cells. TGF-β1 also decreased expression of cdk4 (MBEC, and CCKS1 and HuCCT1) and cdk6 (MBEC, and CCKS1 and HuH28). TGF-β1 did not influence cyclin D2, cyclin D3, and cdk2 expression in both MBEC and any of three ICC cells.
Influence of TGF-β1 on cell proliferative activities of cultured ICC cells after cyclin D1 siRNA transduction
One ICC cell line (HuH28 cells) transfected with cyclin D1 siRNA showed reduced expression of cyclin D1 protein compared to the nontransfected cells and the cells transfected with scrambled siRNA (negative control) (Figure 7), implying successful transfection of cyclin D1 siRNA followed by the destruction of cyclin D1 RNA. TβR-II protein expression was not altered by the transfection of cyclin D1 siRNA or scrambled siRNA (Figure 7).
Transfection of scramble siRNA did not influence cell proliferative activity of HuH28 cells. Transfection of cyclin D1 siRNA resulted in a significant decrease in the cell proliferative activities compared to nontransfected cells and the cells transfected with scrambled siRNA (P<0.05). While the treatment by 0.3?ng/ml of TGF-β1 did not influence proliferative activity of cyclin D1 siRNA-transfected HuH28 cells, 3.0 and 30.0?ng/ml of TGF-β1 significantly inhibited cell proliferation of these cells (P<0.05) (Figure 8). These results indicated that ICC cells acquired responsiveness to TGF-β1 by blocking cyclin D1 expression.
Discussion
It was found in this study that TGF-β1 was expressed in mononuclear inflammatory cells and mesenchymal cells around the stone-containing intrahepatic large bile duct in all cases, and also frequently in hyperplastic, dysplastic, and neoplastic (IPN-B and ICC) biliary epithelial cells. TβR-II was constantly expressed in the biliary epithelium (hyperplasia, dysplasia, IPN-B, and ICC). These results suggested that TGF-β1 liberated from inflammatory and mesenchymal cells and also from biliary epithelial cells around the stone-containing large bile ducts could react to TβR-II expressed on hyperplastic, dysplastic, or neoplastic biliary epithelial cells. Autocrine and paracrine interaction of TGF-β1/TβR-II around ICC and its precursors can give rise to several advantageous effects for ICC and its precursors such as angiogenesis, fibrosis, and suppression of immune system.
We then performed in vitro studies to determine how TGF-β1 influences cell proliferation of non-neoplastic and neoplastic biliary epithelial cells and examine the potential molecular mechanisms. We found that TGF-β1 significantly inhibited the proliferation of MBEC, in which downregulation of cyclin D1, cdk4, and cdk6 might be causally involved. On the other hand, TGF-β1 did not influence the cell-proliferative activities of three cultured human ICC cells. Cyclin D1 expression remained unchanged, even though cdk4 and cdk6 were downregulated. Accordingly, we demonstrated that siRNA inhibition of cyclin D1 expression rendered one ICC cell line sensitive to growth-inhibitory effect of TGF-β1. These results strongly suggested that overexpression of cyclin D1 is a key event for ICC cells attaining TGF-β1-resistance. Indeed, overexpression of cyclin D1 was immunohistochemically detected variably in the nuclei of all cases of biliary dysplasia, IPN-B, ICC with dysplasia or IPN-B, while cyclin D1 was not detectable in biliary hyperplasia or normal bile ducts. Interestingly the labeling index of cyclin D1 was higher in ICC cases than in its precursors (dysplasia and IPN-B), suggesting that overexpression of cyclin D1 is involved in the development and progression of ICC arising in hepatolithiasis.
A similar mechanism for TGF-β-resistance via cyclin D1 overexpression was also reported in human hepatocellular carcinoma (HCC) cells and immortalized human esophageal epithelial cell.25, 26 Jong et al25 reported that HCC cell lines, which were resistant to TGF-β1, showed overexpression of cyclin D1, and the suppression of cyclin D1 expression with antisense cyclin D1 facilitated the growth inhibitory effect of TGF-β1. In addition, Okamoto et al26 reported that immortalized human esophageal epithelial cells became resistant to TGF-β1 after transfection of human cyclin D1 cDNA. Interestingly, transfection of cyclin D1 gene downregulated TβR-II expression in that esophageal epithelial cell line. Okamoto et al26 suggested that cyclin D1 overexpression followed by downregulation of TβR-II might be a key event for those esophageal epithelial cells to obtain TGF-β1-resistance. In this study, transfection of cyclin D1 siRNA did not influence the expression of TβR-II in ICC cells (HuH28), suggesting no close relationship between cyclin D1 expression and TβR-II expression in ICC cells.
In hepatolithiasis, ICC and its precursor lesions are not infrequently encountered,36, 37 and ICC in hepatolithiasis is thought to develop through multistep carcinogenesis.38 At present, at least two pathways of multistep cholangiocarcinogenesis are speculated in hepatolithiasis. The first pathway may be a major pathway through biliary dysplasia showing flat or micropapillary lesion to invasive ICC, usually conventional tubular or papillary adenocarcinoma.38 Another is a unique carcinogenetic pathway from IPN-B to invasive ICC.29 IPN-B is a recently proposed disease entity, and is characterized as prominent papillary proliferation of biliary epithelial cells with gastrointestinal metaplasia and mucin over-production, frequent association with mucinous carcinoma if progressed to invasive cancer, and more favorable prognosis compared to conventional ICC.39, 40 There is now increasing evidence that different genetic abnormalities exist between these two carcinogenetic pathways.41, 42 While no differences in expression of TGF-β1, TβR-II, and cyclin D1, and also genetic mutation of TβR-II were observed between these two precursor lesions and resultant ICC, a potential weakness of this study was that in vitro study was conducted using only human ICC cell lines derived from conventional ICC. So far, cultured cell lines derived from IPN-B or ICC with IPN-B have not been established.
TβR-II was constantly expressed in biliary epithelial cells regardless of atypical degree in 40 cases examined. It was found in this study that no genetic mutations were detectable in exon 3, 5, or 7 of the TβR-II gene in 16 ICC cases. Most mutations of the TβR-II gene reported so far are located in exon 3, 5, and 7.43 As microsatellite regions exist in exon 3 and 7 of the TβR-II gene,44 somatic mutations in these regions may relate to microsatellite instability or replication error.45, 46 Mutations in exon 5 are sporadic and are not associated with replication error.43 Somatic mutations of TβR-II are noticeable in hereditary nonpolyposis colorectal cancer, although these mutations are less frequent in most carcinomas without microsatellite instability.14, 15 Taken together, it seems likely that mutation of exon 3, 5, and 7 of TβR-II is a minor mechanism for TGF-β-resistance in ICC cells.
In conclusion, overexpressed TGF-β1 around ICC and its precursor lesions may exert several advantageous effects for them and be involved in cholangiocarcinogenesis in hepatolithiasis. ICC cells could escape the growth inhibitory effect of TGF-β1 by overexpression of cyclin D1.
References
Massague J . The transforming growth factor-beta family. Annu Rev Cell Biol 1990;6:597–641.
Kingsley DM . The TGF-beta superfamily: new members, new receptors, and new genetic tests of function in different organisms. Genes Dev 1994;8:133–146.
Wrana JL, Attisano L, Wieser R, et al. Mechanism of activation of the TGF-beta receptor. Nature 1994;370:341–347.
Derynck R, Akhurst RJ, Balmain A . TGF-beta signaling in tumor suppression and cancer progression. Nat Genet 2001;29:117–129.
Miyazono K . Positive and negative regulation of TGF-beta signaling. J Cell Sci 2000;113:1101–1109.
Lohr M, Schmidt C, Ringel J, et al. Transforming growth factor-beta1 induces desmoplasia in an experimental model of human pancreatic carcinoma. Cancer Res 2001;61:550–555.
Bellone G, Carbone A, Tibaudi D, et al. Differential expression of transforming growth factors-beta1, -beta2 and -beta3 in human colon carcinoma. Eur J Cancer 2001;37:224–233.
Hasegawa Y, Takanashi S, Kanehira Y, et al. Transforming growth factor-beta1 level correlates with angiogenesis, tumor progression, and prognosis in patients with nonsmall cell lung carcinoma. Cancer 2001;91:964–971.
Ghellal A, Li C, Hayes M, et al. Prognostic significance of TGF beta 1 and TGF beta 3 in human breast carcinoma. Anticancer Res 2000;20:4413–4418.
Norgaard P, Hougaard S, Poulsen HS, et al. Transforming growth factor beta and cancer. Cancer Treat Rev 1995;21:367–403.
Yokomuro S, Tsuji H, Lunz III JG, et al. Growth control of human biliary epithelial cells by interleukin 6, hepatocyte growth factor, transforming growth factor beta1, and activin A: comparison of a cholangiocarcinoma cell line with primary cultures of non-neoplastic biliary epithelial cells. Hepatology 2000;32:26–35.
Lu SL, Zhang WC, Akiyama Y, et al. Genomic structure of the transforming growth factor beta type II receptor gene and its mutations in hereditary nonpolyposis colorectal cancers. Cancer Res 1996;56:4595–4598.
Lu SL, Akiyama Y, Nagasaki H, et al. Mutations of the transforming growth factor-beta type II receptor gene and genomic instability in hereditary nonpolyposis colorectal cancer. Biochem Biophys Res Commun 1995;216:452–457.
Goggins M, Shekher M, Turnacioglu K, et al. Genetic alterations of the transforming growth factor beta receptor genes in pancreatic and biliary adenocarcinomas. Cancer Res 1998;58:5329–5332.
Francis-Thickpenny KM, Richardson DM, van Ee CC, et al. Analysis of the TGF beta functional pathway in epithelial ovarian carcinoma. Br J Cancer 2001;85:687–691.
Riggins GJ, Kinzler KW, Vogelstein B, et al. Frequency of Smad gene mutations in human cancers. Cancer Res 1997;57:2578–2580.
Takagi Y, Koumura H, Futamura M, et al. Somatic alterations of the SMAD-2 gene in human colorectal cancers. Br J Cancer 1998;78:1152–1155.
Paterson IC, Matthews JB, Huntley S, et al. Decreased expression of TGF-beta cell surface receptors during progression of human oral squamous cell carcinoma. J Pathol 2001;193:458–467.
Zhang T, Nanney LB, Peeler MO, et al. Decreased transforming growth factor beta type II receptor expression in intestinal adenomas from Min/+ mice is associated with increased cyclin D1 and cyclin-dependent kinase 4 expression. Cancer Res 1997;57:1638–1643.
Ko TC, Sheng HM, Reisman D, et al. Transforming growth factor-beta 1 inhibits cyclin D1 expression in intestinal epithelial cells. Oncogene 1995;10:177–184.
Geng Y, Weinberg RA . Transforming growth factor beta effects on expression of G1 cyclins and cyclin-dependent protein kinases. Proc Natl Acad Sci USA 1993;90:10315–10319.
Ravitz MJ, Wenner CE . Cyclin-dependent kinase regulation during G1 phase and cell cycle regulation by TGF-beta. Adv Cancer Res 1997;71:165–207.
Carneiro C, Alvarez CV, Zalvide J, et al. TGF-beta1 actions on FRTL-5 cells provide a model for the physiological regulation of thyroid growth. Oncogene 1998;16:1455–1465.
Hu X, Zhang X, Zhong Q, et al. Differential effects of transforming growth factor on cell cycle regulatory molecules in human myeloid leukemia cells. Oncogene 2001;20:6840–6850.
Jong HS, Lee HS, Kim TY, et al. Attenuation of transforming growth factor beta-induced growth inhibition in human hepatocellular carcinoma cell lines by cyclin D1 overexpression. Biochem Biophys Res Commun 2002;292:383–389.
Okamoto A, Jiang W, Kim SJ, et al. Overexpression of human cyclin D1 reduces the transforming growth factor beta (TGF-beta) type II receptor and growth inhibition by TGF-beta 1 in an immortalized human esophageal epithelial cell line. Proc Natl Acad Sci USA 1994;91:11576–11580.
Nakanuma Y, Hoso M, Sanzen T, et al. Microstructure and development of the normal and pathologic biliary tract in humans, including blood supply. Microsc Res Techn 1997;38:552–570.
Nakanuma Y, Sripa B, Vatanasapt V, et al. Intrahepatic cholangiocarcinoma. In: Hamilton SR, Aaltonen LA (eds). WHO Classification of Tumors, Pathology and Genetics, Tumors of Digestive System. IARC Press: Lyon, France, 2000, pp. 173–180.
Chen TC, Nakanuma Y, Zen Y, et al. Intraductal papillary neoplasia of the liver associated with hepatolithiasis. Hepatology 2001;34:651–658.
Saito K, Minato H, Kono N, et al. Establishment of the human cholangiocellular carcinoma cell line (CCKS-1). Kanzo 1993;34:122–129.
Sugawara H, Yasoshima M, Katayanagi K, et al. Relationship between interleukin-6 and proliferation and differentiation in cholangiocarcinoma. Histopathology 1998;33:145–153.
Miyagiwa M, Ichida T, Tokiwa T, et al. A new human cholangiocellular carcinoma cell line (HuCC-T1) producing carbohydrate antigen 19/9 in serum-free medium. In Vitro Cell Dev Biol 1989;25:503–510.
Kusaka Y, Tokiwa T, Sato J . Establishment and characterization of a cell line from a human cholangiocellular carcinoma. Res Exp Med (Berl) 1988;188:367–375.
Katayanagi K, Kono N, Nakanuma Y . Isolation, culture and characterization of biliary epithelial cells from different anatomical levels of the intrahepatic and extrahepatic biliary tree from a mouse. Liver 1998;18:90–98.
Tsang ML, Zhou L, Zheng BL, et al. Characterization of recombinant soluble human transforming growth factor-beta receptor type II (rhTGF-beta sRII). Cytokine 1995;7:389–397.
Nakanuma Y, Terada T, Tanaka Y, et al. Are hepatolithiasis and cholangiocarcinoma aetiologically related? A morphological study of 12 cases of hepatolithiasis associated with cholangiocarcinoma. Virchows Arch A Pathol Anat Histopathol 1985;406:45–58.
Chen MF, Jan YY, Hwang TL, et al. Impact of concomitant hepatolithiasis on patients with peripheral cholangiocarcinoma. Dig Dis Sci 2000;45:312–316.
Terada T, Nakanuma Y, Ohta T, et al. Histological features and interphase nucleolar organizer regions in hyperplastic, dysplastic and neoplastic epithelium of intrahepatic bile ducts in hepatolithiasis. Histopathology 1992;21:233–240.
Shimonishi T, Zen Y, Chen TC, et al. Increasing expression of gastrointestinal phenotypes and p53 along with histologic progression of intraductal papillary neoplasia of the liver. Hum Pathol 2002;33:503–511.
Chen MF, Jan YY, Chen TC . Clinical studies of mucin-producing cholangiocellular carcinoma: a study of 22 histopathology-proven cases. Ann Surg 1998;227:63–69.
Abraham SC, Lee JH, Hruban RH, et al. Molecular and immunohistochemical analysis of intraductal papillary neoplasms of the biliary tract. Hum Pathol 2003;34:902–910.
Abraham SC, Lee JH, Boitnott JK, et al. Microsatellite instability in intraductal papillary neoplasms of the biliary tract. Mod Pathol 2002;15:1309–1317.
Vincent F, Nagashima M, Takenoshita S, et al. Mutation analysis of the transforming growth factor-beta type II receptor in human cell lines resistant to growth inhibition by transforming growth factor-beta. Oncogene 1997;15:117–122.
Takenoshita S, Hagiwara K, Nagashima M, et al. The genomic structure of the gene encoding the human transforming growth factor beta type II receptor (TGF-beta RII). Genomics 1996;36:341–344.
Furuta K, Misao S, Takahashi K, et al. Gene mutation of transforming growth factor beta1 type II receptor in hepatocellular carcinoma. Int J Cancer 1999;81:851–853.
Parsons R, Myeroff LL, Liu B, et al. Microsatellite instability and mutations of the transforming growth factor beta type II receptor gene in colorectal cancer. Cancer Res 1995;55:5548–5550.
Acknowledgements
This work was supported in part by Grants-in-Aid for Intrahepatic Calculi from the Ministry of Health and Welfare, Japan.
Author information
Authors and Affiliations
Corresponding author
Rights and permissions
About this article
Cite this article
Zen, Y., Harada, K., Sasaki, M. et al. Intrahepatic cholangiocarcinoma escapes from growth inhibitory effect of transforming growth factor-β1 by overexpression of cyclin D1. Lab Invest 85, 572–581 (2005). https://doi.org/10.1038/labinvest.3700236
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/labinvest.3700236
Keywords
This article is cited by
-
Blocking ERK1/2 signaling impairs TGF-β1 tumor promoting function but enhances its tumor suppressing role in intrahepatic cholangiocarcinoma cells
Cancer Cell International (2017)
-
Genome-wide screen identified let-7c/miR-99a/miR-125b regulating tumor progression and stem-like properties in cholangiocarcinoma
Oncogene (2016)
-
Clinicopathological significance of growth factors and their receptors as potential therapeutic targets for biliary tract carcinoma
Journal of Hepato-Biliary-Pancreatic Sciences (2012)
-
Prospects of RNA interference therapy for cancer
Gene Therapy (2006)