PDCD5 expression predicts a favorable outcome in patients with hepatocellular carcinoma
- Da-Zhi Fu
- Ying Cheng
- Hui He
- Hai-Yang Liu
- Yong-Feng Liu
- Corresponding author:
- Yong-Feng Liu [ email@example.com ]
Published online on: Wednesday, June 26, 2013
- Pages: 821-830 DOI: 10.3892/ijo.2013.1993
Liver cancer in men is the fifth most frequently diagnosed cancer worldwide but the second most frequent cause of cancer death. An estimated 748,300 new liver cancer cases and 695,900 cancer deaths occurred worldwide in 2008 (1). Half of these cases and deaths were estimated to occur in China (2). Among primary liver cancers, hepatocellular carcinoma (HCC) represents the major histological subtype, accounting for 70–85% of the total liver cancer burden worldwide (3).
TF-1 apoptosis-related gene 19 (TFAR19) was first cloned as an upregulated gene from TF-1 cells undergoing apoptosis following serum withdrawn by Liu et al(4) in the Peking University Center for Human Disease Genomics in 1999, then designated as programmed cell death 5 (PDCD5) by International Human Gene Nomination Committee (GenBank accession no. AF014955). PDCD5 gene is located on chromosome 19q12-q13.1 (5) and the integrated PDCD5 protein contains 125 amino acid (aa) residues (6). Decreased expression of PDCD5 has been characterized for human tumors including breast cancer (7), gastric cancer (8), astrocytic glioma (9) and chronic myelogenous leukemia (10). The scientists in the Peking University Center for Human Disease Genomics established an ELISA method for detecting soluble PDCD5 protein (11). Wang et al(12) illustrated a significant elevation of PDCD5 concentrations in both plasma and synovial fluid of knee rheumatoid arthritis (RA) patients compared to osteoarthritis (OA) patients and the control plasma concentrations. The serum PDCD5 levels in breast cancer, gastrointestinal tract cancer and lung cancer patients were separately compared with healthy persons by Wang et al(13). However, the significance of serum PDCD5 and its changes in various cancers await further investigations.
Xu et al(14) demonstrated that PDCD5 interacts with Tip60, enhances the histone acetylation and p53 K120 acetylation and promotes the expression of Bax, consequently accelerating apoptosis. In their recent study, novel evidence demonstrated that PDCD5 is a p53 regulator during gene expression and cell cycle (15). Li et al(16) found that PDCD5 promotes cisplatin-induced apoptosis of glioma cells via activating mitochondrial apoptotic pathway. Han et al(17) confirmed that PDCD5 shows a greater inhibitory effect on the Ras/Raf/MEK/ERK signaling pathway in the human osteosarcoma cell line MG-63. However, the molecular mechanisms underlying PDCD5 functions during cell growth, proliferation and apoptosis remain largely unclear.
In this study, we first demonstrate that PDCD5 expression is correlated with clinicopathological features and patient survival and it may be a useful predictor of prognosis in patients with HCC after surgical resection. Second, we compared the PDCD5 levels in peripheral blood serum from cancer patients with matched normal volunteers. The susceptibility of HCC cells to human PDCD5 was also investigated in vitro.
Materials and methods
Cell culture and tumor specimens
Human liver cancer cell lines, HepG2 and Hep3B, were cultured in DMEM (Hyclone, Logan, UT, USA) containing 10% fetal bovine serum (Invitrogen Gibco, Carlsbad, CA, USA) and incubated in a 5% CO2 incubator at 37°C. Liver cancer tissue specimens and their adjacent normal liver tissues were derived from 56 patients undergoing surgical resection of primary hepatocellular carcinoma without prior chemotherapeutic treatment or radiotherapy. The adjacent non-malignant tissue was ≥1-cm distance from the tumor margin. Resections were performed at Department of General Surgery, First Affiliated Hospital of China Medical University from January 2008 to December 2012. All patients approved the use of tumor tissues for clinical research and China Medical University Ethics Committee approved the research protocols. Basic patient information is summarized in Table I.
PDCD5 expression associated with demographic and biological parameters in 56 hepatocellular carcinoma samples.
Quantitative real-time PCR
Total RNA was isolated using an RNeasy Mini kit (Biomed, Beijing, China). First strand cDNA was reverse transcribed with 1 μg of total RNA, using Takara Reverse Transcription kit (Takara, Dalian, China) and oligo(dT) 15 primers (Takara). The resultant cDNA was then used for quantitative PCR reactions. The PDCD5 primers were: sense: 5′-CTGAGGAGACAGAGGCTGGC-3′ and antisense: 5′-TTTCTGCTTCCCTGTGCTTTG-3′. The housekeeping genes, GAPDH and β-actin, were used as internal controls for normalization of the results. The GAPDH primers were: sense: 5′-AGAAGGCTGGGGCTCATTTG-3′ and antisense: 5′-AGGGGCCATCCACAGTCTTC-3′. The β-actin primers were: sense: 5′-CTCCCTGGAGAAGAGCTACGA-3′ and antisense: 5′-GTGGGACTTCCAGAACTGCA-3′. Amplification of PDCD5, GADPH and β-actin was performed with 1 cycle at 95°C for 10 min and 40 cycles of 95°C for 15 sec and 60°C for 60 sec. Calculation of the relative expression of each transcript was performed using the 2−ΔΔCt method (18).
RNA isolation and reverse transcriptase-polymerase chain reaction (RT-PCR)
Total RNA was isolated from HepG2 and Hep3B cells using the RNeasy Mini kit (Biomed, Beijing, China). First strand cDNA was reverse transcribed with 1 μg total RNA, using the Takara Reverse Transcription kit (Takara) and oligo(dT)-15 primers (Takara) according to the manufacturer′s instructions. The primers of PDCD5 and GAPDH were used as described above. PCR amplification of cDNA was performed in 20 μl mixtures. Finally, products were resolved by 1.5% agarose gel electrophoresis and visualized by ethidium bromide staining and a UV imaging system (UVP, LLC, Upland, CA, USA).
Immunohistochemical staining (IHC)
IHC of 4-μm sections of paraffin-embedded specimens was performed using the anti-PDCD5 polyclonal antibody (Beijing Biosea Biotechnology, Beijing, China). Briefly, after deparaffinization and hydration, the endogenous peroxidase activity was quenched by a 30-min incubation in a mixture of 0.3% hydrogen peroxide solution in 100% methanol. The sections were blocked for 2 h at room temperature with 1.5% blocking serum in PBS and incubated with anti-PDCD5 antibody (1:200 dilution) at 4°C in a moist chamber overnight, followed by incubation with Envision reagent (Dako, Carpinteria, CA, USA) and color development in 3,3′-diaminobenzidine tetrahydrochloride (DAB, Sigma-Aldrich, Carlsbad, CA, USA). The slides were then lightly counterstained with hematoxylin, dehydrated with ethanol, cleaned with xylene and mounted. Adjacent non-cancer tissues were used as controls. Sections treated without primary antibodies were used as negative controls. The positive percentage of counted cells was graded semi-quantitatively according to a four-tier scoring system: negative (−), 0–5%; weakly positive (+), 6–25%; moderately positive (++), 26–50%; and strongly positive (+++), 51–100%.
Preparation of blood samples and measurement of PDCD5 and AFP in serum
Peripheral blood was obtained from 58 patients with HCC and 58 healthy volunteers. Samples were clotted for 30 min and then centrifuged for 10 min at 1000 × g. All samples were then frozen and stored at −80°C until required for assay. Concentration of PDCD5 in serum was assayed using enzyme-linked immunosorbent assay (ELISA) kit for PDCD5 (USCN Life Science Inc., Houston, TX, USA). Concentration of AFP in serum was measured using an ELISA kit from Diagnostic Automation/Cortez Diagnostics Inc (Calabasas, CA, USA).
Plasmid and transfection
The plasmid, pcDNA3.1-PDCD5, was kindly provided by Mr. Xiao-Rui Han (China Medical University, Shenyang). Transfection of the plasmid into HepG2 cells or Hep3B was performed using Lipofectamine™ 2000 (Invitrogen) according to the manufacturer’s instructions. Cell lines after transfection were named HepG2-T and Hep3B-T. Cell lines transfected with pcDNA3.1 was used as a mock and named HepG2-M and Hep3B-M.
Transfected cells were washed with PBS, fixed in 4% paraformaldehyde, permeabilized in 1% Triton X-100 for 5 min and blocked with 5% bovine serum albumin in PBS containing 0.5% Triton X-100 for 1 h. PDCD5 expression was detected using anti-PDCD5 (Beijing Biosea Biotechnology) antibody for 1 h at room temperature. Cells were washed with PBS and incubated with appropriate secondary fluorophore-conjugated antibody for 1 h at room temperature, washed with PBS and mounted using SlowFade® Gold Antifade reagent (Invitrogen). Secondary antibody used for detection of PDCD5 was Alexa Fluor® 594 Donkey Anti-Goat IgG (H+L) (Invitrogen).
Evaluation of cell viability by MTT assay
Cell viability was assayed using 3-(4,5-dimethylthiazolyl)-2,5-diphenyltetrazoliumbromide (MTT) assays (Sigma). Briefly, cells were plated in 96-well plates (1,500 cells per well). After 24 h, 0.5 mg/ml MTT was added to each well. Four hours later, cells were lysed with dimethyl sulfoxide (DMSO) and absorbance rates were measured at 550–560 nm using a microplate reader (Bio-Rad, Hercules, CA, USA). Proteasome inhibitor, MG132, purchased from Calbiochem (La Jolla, CA, USA), was used as a control in the following experiments.
For apoptosis detection, HepG2 cells, HepG2-M cells, HepG2-T cells, HepG2 treated with MG132, Hep3B cells, Hep3B-M cells, Hep3B-T cells and Hep3B cells treated with MG132 were washed in PBS, fixed, permeabilized and subjected to TUNEL labeling using an In Situ Cell Death Detection kit (Keygen, Nanjing, China) according to the manufacturer’s protocol. After counterstaining with DAPI (1 μg/ml), photographic images were taken using an Olympus CX71 fluorescence microscope (Olympus, Tokyo, Japan). TUNEL-positive nuclei were stained green and all other nuclei were stained blue (19).
Cell apoptosis assay
Cells (5×105) were collected without EDTA and washed with PBS. A 500-μl binding buffer, 5 μl Annexin V-FITC and 5 μl propidium iodide (PI) were added into the suspension in this order and mixed at room temperature in dark for 10 min. The examination was performed by flow cytometry within 1 h.
Cell cycle assay
Cells seeded on 6-well plates were treated and then collected. After being washed with PBS three times, the cell suspension was fixed with 70% ethanol, incubated with RNAse A at 37°C. After staining with 400 μl PI, the suspension was evaluated by flow cytometry.
In vitro wound healing assay
Cells were grown in a 6-well dish. A confluent monolayer of cells was scratched with a 200-μl pipette tip to create a wound. Cells were washed twice with PBS and then supplemented with medium and incubated for 4 h at 37°C. Cell migration into the wounded area was monitored microscopically. Images were captured at the interface of the unwounded and wounded areas.
26S proteasome activity assay
26S proteasome function was assayed as described previously (20). The assay is based on detection of the fluorophore 7-amino-4-methylcoumarin (AMC) after cleavage from the labeled substrate Suc-LLVY-AMC (Boston Biochem, Boston, MA, USA). These fluorogenic proteasome substrates were added to the cell lysate at a final concentration of 80 μM in 1% DMSO. ATP-dependent cleavage activity was monitored continuously by detection of free 7-amido-4-methylcoumarin using a microplate reader (Bio-Rad) at 380/460 nm, at 37°C.
Western blot analysis
The total protein was extracted from human liver cancer cell lines and liver tissues using RIPA buffer (Sigma). The protein concentration was determined with BCA Protein Assay kit (Pierce, Rockford, IL, USA). For performing nitrocellulose membrane blotting, 60 μg cell lysates were separated on a 10% SDS-PAGE. The blotted membranes were blocked with 5% BSA in TBST for 2 h at room temperature and incubated with each primary antibody overnight. The primary antibodies were PDCD5 (Abcam, Cambridge, UK) and β-actin (Santa Cruz Biotechnology, Santa Cruz, CA, USA). The reaction was followed by probing with peroxidase-coupled secondary antibodies at dilutions ranging from 1:1,000 to 1:2,000 (Amersham Biosciences, Needham, MA, USA) and binding results were visualized by enhanced chemiluminescence (Amersham Pharmacia, Piscataway, NJ, USA).
Statistical analyses were performed using SPSS 15.0 software (SPSS, Chicago, IL, USA). Comparisons were made using χ2 tests, the Wilcoxon signed-rank test and the t-test. Overall survival was analyzed using the Kaplan-Meier method and the significance of differences in survival rates was estimated using the log-rank test. Values of P<0.05 were considered significant.
PDCD5 is downregulated in HCC tissues compared with normal tissues
To initially confirm the roles of PDCD5 expression in human liver cancer development and progression, we assayed the expression of PDCD5 in 56 pairs of human hepatocellular carcinomas and corresponding adjacent normal tissues. Levels of PDCD5 mRNA and protein in the hepatoma tissue were significantly lower than those in corresponding adjacent non-cancer tissue (Fig. 1A and B; P<0.05). In Fig. 1C, the results of immunohistochemical staining showed that positive staining was seen in the cytoplasm of the normal cells, in contrast, almost no positive cells were seen in cancer tissue. Moreover, the PDCD5 expression was correlated statistically with HBV infection (P=0.030), tumor number (P=0.030) and lymph node metastasis (P=0.011). There was no significant correlation between PDCD5 expression and age, sex, tumor number, tumor size, differentiation and portal invasion (Table I, P>0.05). HCC patients with PDCD5 expression were associated with a significantly better survival rate than those without PDCD5 expression (Fig. 2, P=0.038).
(A) The level of PDCD5 mRNA was measured in specimens by using real-time PCR. GADPH and β-actin were used as internal controls. (B) Representative results of two pairs of HCC and corresponding normal tissue by western blotting. β-actin was used as an internal control. (C) Immunohistochemical staining for PDCD5 protein in specimens. PDCD5 was stained yellow with granules and localized to the cytoplasm. The nuclei were counterstained with hematoxylin. N, normal; C, cancer; NC, negative control.
Kaplan-Meier curves for cumulative survival rate of the patients with HCC according to the PDCD5 expression.
The serum levels of PDCD5 and AFP detection in patients with HCC
The serum PDCD5 contents in 58 HCC patients ranged from 4.41 pg/ml to 1.72 ng/ml with a median of 421.83±12.52 pg/ml. There was statistical significance compared with the serum PDCD5 level in healthy persons (Fig. 3A, P<0.05). Serum AFP levels in the HCC patients (6.24 pg/ml to 1.53 ng/ml) were significantly higher than that in the control group (32.67 pg/ml to 2.46 ng/ml) (Fig. 3B, P<0.05). The serum levels of PDCD5 and AFP in 58 HCC patients were significantly positively correlated (r=0.913) (Fig. 3C, P<0.05).
PDCD5 and AFP in serum of HCC patients and healthy controls. (A) Serum PDCD5 levels from patients with HCC (n=58) vs healthy controls (n=58). (B) Serum AFP levels from patients with HCC (n=58) vs healthy controls (n=58). (C) Positive correlation between serum levels of PDCD5 and AFP in HCC patients (n=58).
Establishment of PDCD5-overexpressing HepG2 and Hep3B cells
To investigate further the phenomenon and mechanism of the PDCD5-mediated regulation of liver cancer cell growth and metastasis, cell lines, HepG2 and Hep3B, were selected for PDCD5 gene enhancement. After pcDNA3.1-PDCD5 was transfected into the two hepatoma cell lines, PDCD5 mRNA and protein levels were significantly increased compared to untransfected cells by using RT-PCR and western blotting, respectively (Fig. 4A and B). Immunofluorescence analysis showed PDCD5 was localized in the cytoplasm of transfected cells (Fig. 4C). These results collectively suggested that the transfection was successful.
The levels of PDCD5 protein and mRNA were measured in HCC cell lines. (A) The mRNA level of PDCD5 was determined by RT-PCR. GAPDH was used as an internal control. (B) The expression of PDCD5 protein was determined by western blotting of HepG2 cells and Hep3B cells and the two cells transfected with pcDNA3.1-PDCD5. β-actin expression was used as an internal control. (C) Detection of PDCD5 in transfected and untransfected cells by immunofluorescence. PDCD5 protein was located predominantly in the cytoplasm.
PDCD5 displays antitumor activity in liver cancer cells
Since PDCD5 mRNA and protein levels are decreased in liver cancer tissues and cells, we determined whether its exogenous expression would reduce tumorigenicity of liver cancer cells. The MTT assay showed that the proliferation rate of PDCD5-expressing cells was decreased compared to untransfected and mock-transfected cells (Fig. 5A, P<0.05). TUNEL assay confirmed that the number of apoptotic cells in the transfected group was significantly more than untransfected group and mock-transfected group (Fig. 5B). To quantify apoptotic cells, Annexin V-FITC and PI double staining was performed. In cells expressing PDCD5, the apoptotic ratio was 3–6 times higher than that of untransfected and mock-transfected cells. We determined that the percentage of apoptosis in PDCD5-expressing HepG2 cells was 3.86%, significantly higher compared to untransfected (0.73%) and mock-transfected (1.12%) HepG2 cells (Fig. 5C, P<0.05). The apoptotic percentage of PDCD5-expressing Hep3B cells was 3.75% compared to untransfected (1.23%) and mock-transfected (1.34%) Hep3B cells (Fig. 5C, P<0.05). PI staining of cells revealed that PDCD5-expressing cells were arrested in G1 phase (Fig. 5D, P<0.05). We determined the mobility change in PDCD5-expressing cells using the wound healing assay. The percentage of wound closure of PDCD5-positive cells was decreased when compared to untransfected and mock-transfected cells (Fig. 5E, P<0.05).
The antitumor roles of PDCD5 protein in HCC cells. (A) MTT assays were performed to determine the proliferation ratio of HCC cells with PDCD5 transfection compared with untransfected ones. (B) Representative TUNEL staining images of transfected cells and untransfected ones. Apoptotic cells with DNA fragmentation were stained positively as green nuclei. (C) The proportion of apoptotic cells (early apoptosis) was determined by double-staining with Annexin V/FITC and PI. (D) Cells were stained with PI to analyze the cell cycle distribution of each cell type by flow cytometry. (E) Wound closure was quantified in the regions flanked by dotted lines. (F) Inhibitory effect of PDCD5 on proteasome was determined by using a microplate reader. MG132 was used as a control in each experiment. Each experiment was performed in triplicate and was repeated three times. HepG2-M, HepG2 transfected with pcDNA3.1; HepG2-T, HepG2 transfected with pcDNA3.1-PDCD5; Hep3B-M, Hep3B transfected with pcDNA3.1; Hep3B-T, Hep3B transfected with pcDNA3.1-PDCD5.
PDCD5 inhibits proteasome activity in liver cancer cells
In order to determine whether PDCD5 could impact on the proteasome, we compared the response of MG132 treated liver cancer cells with PDCD5 treated cells. The proteasome activity of both PDCD5-expressing HepG2 cells and PDCD5-expressing Hep3B cells was lower than that of untransfected and mock-transfected cells (Fig. 5F, P<0.05). HepG2 cells and Hep3B cells after MG132 treatment also showed increased apoptosis, G1 arrest and decreased mobility. Thus, the results showed that MG132 has the same effect as PDCD5 in liver cancer cells (Fig. 5, P<0.05). These data collectively indicate that PDCD5 suppressed HCC cells via inhibition of proteasome activity.
Several pieces of evidence have suggested that the expression of PDCD5 protein is downregulated in some human tumors, such as breast cancer (7), gastric cancer (8) and astrocytic glioma (9). In the study of Xu et al(21), gene expression profiles of HCC and non-HCC, based on cDNA arrays or RT-PCR, reflected a number of genes with relatively high expression in non-HCC, including PDCD5. However, the clinical significance of PDCD5 expression in HCC has not been well characterized. In this study, we confirmed both PDCD5 mRNA and protein were significantly higher in normal matched tissues than that in HCC tissues. Low expression of PDCD5 in chondrosarcoma samples was significantly correlated with anatomical location and histological grade, but not with age and gender (22). The expression of PDCD5 in gliomas was correlated significantly with the pathological grade. However, we found that the PDCD5 expression was correlated statistically with HBV infection, tumor number and lymph node metastasis. The discrepancy might be attributable to clinicopathological characteristics of the subjects and grouping methods. Previous studies have documented that PDCD5 expression can be predictive for the prognosis of patients with several tumors (8,9,22). We performed Kaplan-Meier analysis and confirmed PDCD5 protein was associated with the overall survival of patients with HCC. Therefore, it is implied that PDCD5 may be a favorable biomarker for the prognosis of patients with HCC. Since the sample size in this study may be considered small, further investigation of a larger patient population is necessary to confirm its clinical value and prognostic evaluation in HCC. α-fetoprotein (AFP), is still the only serological marker presently available for routine screening in most parts of the world. High levels of AFP in fully developed hepatocarcinoma or in serum of the host are associated with more aggressive behavior and increased anaplasia (23,24). In this study, the concentrations of PDCD5 and AFP in serum were lower in HCC patients than that in healthy controls and confirmed that the levels of PDCD5 and AFP were significantly positively correlated. A strong correlation between PDCD5 and IL-17 levels in serum of RA patients has been determined in a previous study (25). Wang et al(13) found decreased expression of PDCD5 in peripheral blood of breast cancer, lung cancer and gastrointestinal cancer, however, the PDCD5 levels in cancer patients are not statistically different from that of normal persons. The level of PDCD5 in serum may be used as a novel marker for HCC.
Previous studies have demonstrated that PDCD5 is an apoptosis-promoting molecule that is upregulated in cells undergoing apoptosis (4,14,26,27). Likewise, blocking the activity of PDCD5 by introducing an anti-PDCD5 antibody or siRNA against PDCD5 could suppress etoposide or Bax- induced apoptosis of tumor cells (28,29). In MTT assay, the proliferation ratio of transfected cells was reduced compared to untransfected ones in our study. Correspondingly, transfected cells exhibited a higher apoptotic ratio than untransfected cells by TUNEL assay and Annexin V/PI double staining. Collectively, these results suggest that PDCD5 may have a suppressive role in HCC cells.
The mechanisms involved in PDCD5 expression are still being investigated. PDCD5 positively regulates Tip60, a transcriptional coregulator, which in turn, promotes p53 acetylation, leading to enhanced p53-dependent apoptosis (14). Another study showed that apoptotic potential of PDCD5 is linked with CK2 phosphorylation (30). It has also been shown that PDCD5 can enhance TAJ/TROY-induced paraptosis-like cell death (26). Han et al(17) found that PDCD5 mediates antitumor effects in the osteosarcoma cell line by suppressing the Ras/Raf/MEK/ERK signaling pathway. An et al(31) found that myocardial high PDCD5 overexpression results in dilated cardiomyopathy and heart failure accompanied by dramatically enhanced autophagy. Interesting, the major finding in the present study is that PDCD5 overexpression is involved in proteasome inhibition. This is supported by the fact that, PDCD5 showed the same antitumor activity as the proteosome inhibitor, MG132. The proteasome activity of transfected cells was lower than untransfected ones. Proteasome inhibition has gained interest as anticancer therapy (32). Proteasome inhibition disturbs the critical intracellular balance between proapoptotic and antiapoptotic signals shifting it towards tumor growth inhibition, apoptosis and decreased metastasis (33).
In conclusion, we have demonstrated that a decreased expression of PDCD5 correlated significantly with HBV infection, tumor number and lymph node metastasis. Although previous studies have provided insightful mechanisms of PDCD5 involved in intrinsic or extrinsic apoptotic pathways, our results showed evidence that PDCD5 is involved with proteasome inhibition. PDCD5 may serve as a novel therapeutic target for the treatment of hepatocellular cancer.
We thank Dr Miao Yu for technical assistance.