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Open Access

Downregulation of castor zinc finger 1 predicts poor prognosis and facilitates hepatocellular carcinoma progression via MAPK/ERK signaling

  • Ji-Long Wang1,
  • Meng-yuan Yang2,
  • Shuai Xiao1, 3,
  • Bo Sun1,
  • Yi-Ming Li1 and
  • Lian-Yue Yang1, 3Email author
Journal of Experimental & Clinical Cancer Research201837:45

https://doi.org/10.1186/s13046-018-0720-8

Received: 16 December 2017

Accepted: 22 February 2018

Published: 5 March 2018

Abstract

Background

Castor zinc finger 1 (CASZ1) plays critical roles in various biological processes and pathologic conditions, including cancer. However, the prognostic importance and biologic functions of CASZ1 in hepatocellular carcinoma (HCC) are still unclear.

Methods

qRT-PCR, western blot and immunohistochemistry analyses were used to determine CASZ1 expression in HCC samples and cell lines. The clinical significance of CASZ1 was assessed in two independent study cohorts containing 232 patients with HCC. A series of in vitro and in vivo experiments were performed to explore the role and molecular mechanism of CASZ1 in HCC progression.

Results

Here we report that CASZ1 expression was downregulated in HCC tissues and cell lines. Low CASZ1 expression was closely correlated with aggressive clinicopathological features, poor clinical outcomes and early recurrence of HCC patients. Moreover, overexpression of CASZ1 in HCCLM3 cells significantly inhibited cell proliferation, migration, invasion in vitro and tumor growth and metastasis in vivo, whereas silencing CASZ1 significantly enhanced the above abilities of PLC/PRF/5 cells. Further mechanism study indicated that these phenotypic changes were mediated by MAPK/ERK signaling pathway and involved altered expression of MMP2, MMP9 and cyclinD1. Finally, we proved that CASZ1 exerted its tumor-suppressive effect by directly interacting with RAF1 and reducing the protein stability of RAF1.

Conclusions

Our study for the first time demonstrated that CASZ1 is a tumor suppressor in HCC, which may serve as a novel prognostic predictor and therapeutic target for HCC patients.

Keywords

Castor zinc finger 1Hepatocellular carcinomaProgressionMAPK/ERKRAF1

Background

Hepatocellular carcinoma (HCC) is the second leading cause of cancer-related death worldwide, with more than 50% of HCC cancer cases and deaths occurred in China [1, 2]. Despite recent progress in HCC prevention, diagnosis and intervention, patients with HCC still have a very dismal long-term survival due to the high incidence of recurrence and metastasis [3, 4]. During the past decades, remarkable advances have been made to explore the pathogenesis of HCC [57]; but the underlying mechanisms responsible for HCC recurrence and metastasis are still largely unclear. Therefore, more reliable biomarkers for predicting relapse and understanding the mechanisms of HCC metastasis need to be developed urgently.

Castor zinc finger 1 (CASZ1) was initially characterized as a neural fate-determination gene [8], which plays critical roles in cell differentiation, as well as neural and cardiac developmental processes in Drosophila and Xenopus models [915]. In addition, CASZ1 promotes angiogenic sprouting and lumen morphogenesis through regulating endothelial cell contractility and adhesion [16, 17]. Recently, the importance of CASZ1 in tumorigenesis is becoming increasingly recognized. Aberrant fusion transcript of CASZ1 has been reported in colorectal cancer [18] and bladder cancer [19]. CASZ1 is downregulated and functions as a crucial tumor suppressor in neuroblastoma [20, 21]. In contrast, CASZ1 is highly expressed and responsible for cell migration and invasion in epithelial ovarian cancer [22], which indicated CASZ1 had different expression patterns and functions in various human cancers. Given the potential significance of CASZ1 in cancer pathobiology, its clinical relevance and potential role in human HCC deserves to be investigated.

In the present study, we found that CASZ1 was markedly downregulated in HCC tissues and cell lines, and low expression of CASZ1 was closely associated with aggressive clinicopathologic features, poor prognosis and early recurrence of HCC patients. Overexpression of CASZ1 suppressed, while silencing CASZ1 promoted HCC cell proliferation, migration and invasion both in vitro and in vivo. Furthermore, we demonstrated that CASZ1 inhibited MAPK/ERK signaling activity through direct downregulation of RAF1. Therefore, our results suggested that CASZ1 plays important suppressive roles in HCC progression and may serve as a potential prognostic predictor and therapeutic target for HCC.

Methods

HCC samples and follow-up

One hundred thirty-two HCC specimens in training cohort were randomly selected from Xiangya Hospital of Central South University between January 2007 and June 2010. Another 100 HCC samples in validation cohort were selected from the Affiliated Cancer Hospital of Xiangya School of Medicine between November 2008 and December 2011. The details of sample collection were shown in Additional file 1: Figure S1, while the baseline characteristics of these patients were described in Additional file 2: Table S1. All research protocols strictly complied with REMARK guidelines for reporting prognostic biomarkers in cancer [23]. Follow-up procedures were conducted as described in our previous study [24]. Frozen normal liver tissues (NLs), HCC tissues and adjacent non-tumor liver tissues (ANLTs) were used for qRT-PCR and western blot analysis.

Cell lines and cell culture

MHCC97-L, MHCC97-H and HCCLM3 were kindly provided by the Liver Cancer Institute of Fudan University, Shanghai, China. PLC/PRF/5, Hep3B and HepG2 cells were purchased from the American Type Culture Collection (ATCC, Manassas, VA). L02, SMMC7721 and Huh7 cells were purchased from the Cell Bank of Typical Culture Preservation Committee of Chinese Academy of Science, Shanghai, China. Cells were maintained in Dulbecco’s Modified Eagle’s Medium (Biological Industries, Kibbutz Beit Haemek, Israel) supplemented with 10% fetal bovine serum (FBS, Biological Industries), 100 μg/mL streptomycin, and 100 U/mL penicillin (Hyclone, Logan, UT) at 37 °C in a humidified atmosphere with 5% CO2.

RNA extraction and quantitative real-time PCR

Total RNA was extracted from tissues or cells with TRIzol reagent (Invitrogen,Carlsbad, CA). Reverse transcription were performed using an Advantage RT-for-PCR Kit (Takara, Dalian, China). qRT-PCR analysis was done using SYBR®Green Real time PCR Master Mix assay kit (Takara) in a 7300 Real-Time PCR system (Applied Biosystems Inc., Foster City, CA) with the following primers (5′ → 3′): CASZ1 forward, CCTCCCTGTCCTT CAACACT and reverse, GACGGCTGGTTTATCTGTGG; RAF1 forward, CCGAACAAGCAAAGAACAGTG and reverse, GACGCAGCATCAGTATTCCAAT. GAPDH was used as endogenous control.

Protein extraction and western blot

Tissues or cells were lysed with RIPA buffer (Pierce, Rockford, IL) supplemented with protease inhibitors. Protein concentration was measured using a BCA protein assay (Thermo Scientific, Rockford, IL). Protein lysates, suspended in loading buffer, were separated on 10% SDS-polyacrylamide gels and transferred onto PVDF membranes (Millipore, Belford, MA). Then these membranes were blocked with 5% skim milk at room temperature for 1 h, and incubated with primary antibodies at 4 °C overnight. After washed, they were incubated with suitable HRP-conjugated secondary antibody at room temperature for 30 min and detected using an enhanced chemiluminescence (ECL) kit (Thermo Scientific). Antibodies for CASZ1, ERK and p-ERK were obtained from Abcam (Cambridge, MA), for RAF1, cyclinD1, E-cadherin, N-cadherin and Vimentin were purchased from Santa Cruz Biotechnology (Santa Cruz, CA), for MMP2 and MMP9 were purchased from Affinity Biosciences (Cincinnati, OH). β-actin antibody and corresponding secondary antibodies were purchased from Zhongshan Golden Bridge Biotechnology (ZSGB, Beijing, China).

Immunohistochemical (IHC) analysis and scoring

The tissue sections were deparaffinized in xylene and rehydrated using a series of graded alcohols. Antigen retrieval was performed by microwave treatment in citrate buffer (pH 6.0) for 15 min. Endogenous peroxidase activity was inactivated using hydrogen peroxide (0.3%). After washed, the sections were blocked with 10% normal goat serum and incubated with primary antibody at 4 °C overnight. Signal was visualized using standard protocols with HRP conjugated secondary antibody and DAB (ZSGB) as the substrate. For negative controls, sections were incubated with normal goat serum rather than primary antibody. Finally, the sections were counterstained with hematoxylin and dehydrated in ethanol before mounting. The IHC score of target proteins was independently evaluated by two investigators according to the proportion and intensity of positive cells within five randomly selected fields per slide (magnification, × 400). The intensity was assessed by four grades: 0 for none; 1 for weak; 2 for moderate; 3 for strong. The percentage of positive cells was divided into five degrees: 0, no positive tumor cells; 1 for ≤5%; 2 for 6–25%; 3 for 26–75%; 4 for ≥76%. Immunoreactive score was calculated by multiplying the staining extent score with the intensity score. High expression was defined as a staining index score > 4, while low expression was defined as a staining index score ≤ 4 [25].

Transfection and clone selection

The ectopic expression and knockdown lentivirus as well as control lentivirus for CASZ1 and RAF1 were all purchased from GenePharma (Suzhou, China). Transfection was performed according to the manufacturer’s instructions. Puromycin (2 μg/mL) was used to select stable clones. The sequences of shRNA are listed as follows (5′ → 3′): CASZ1-sh1: GCCGTCACTGAAGATGTAAAC; CASZ1-sh2: GCCAGTTCTACGGACAGAAGA; CASZ1-sh3: GCCCAGCAACGAATCAAATGG; RAF1-sh1: ATCAATTCAAGAGATTGATGT; RAF1-sh2: ACTTTTTCAAGAGAAAAGTTC; RAF1-sh3: CAATATTCAAGAGATATTGTT.

MTT assay and colony formation assay

For MTT assay, 5 × 103 cells were seeded in 96-well plates, incubated for 0–7 days, stained with MTT, and absorbance values were determined at 570 nm using a spectrophotometer. The relative cell number was normalized by the absorbance from the control cells. For colony formation assays, 500 cells were seeded per well in 6-well plates and cultured for 14 days. The colonies were fixed with 4% paraformaldehyde and stained with 1% crystal violet. Only colonies containing more than 50 cells were counted [26].

Cell cycle analysis

5 × 105 cells were seeded in 6-well plates and incubated for 24 h. Then cells were harvested and fixed with cold 70% ethanol at − 20 °C overnight. After washing, cells were stained in a solution containing PI (0.5 mg/mL) and RNase A (10 mg/mL). Then cells were filtered through a 70 μM cell strainer immediately prior to flow cytometry, which was carried out on a FACS caliber flow cytometer (BD Biosciences, San Jose, CA).

Wound healing and transwell invasion assay

For wound healing assay, 5 × 105 cells were seeded into 6-well plates and grown to confluence. Mitomycin C (10 μg/mL) was used to suppress cell proliferation before scratching [27]. Wounds were created by scraping the confluent cell monolayers with a 10 μL pipette tip. After extensively rinsed to remove cellular debris, cells were cultured in serum-free medium. The wound closure rate was monitored every 12 h and images were taken using an inverted microscope TE-2000S (Nikon, Tokyo, Japan). Transwell invasion assay was performed in a 24-well transwell plate with 8-μm polyethylene terephthalate membrane fiters (Corning Costar Corp, Corning, NY). 1 × 105 cells in 200 μL of serum-free medium were added to the upper chambers, which contained matrigel-coated membranes (BD Biosciences). Each lower chamber was filed with 500 μL medium with 10% FBS. After 18 h or 24 h of incubation, cells that invaded to the bottom chamber were fixed with 4% paraformaldehyde and stained with 0.1% crystal violet. Invasive cells were counted in five randomly chosen fields (magnification, × 200) per well.

Cancer 10-pathway reporter arrays

A Cignal Finder 10-Pathway Reporter Array (SABiosciences, Valencia, CA) was performed to explore the signaling pathways that were regulated by CASZ1 in HCC cells. The assay was conducted according to the manufacturer’s protocol. Relative firefly luciferase activity was calculated and normalized to the constitutively expressed Renilla luciferase. Experiments were done in triplicates.

Co-immunoprecipitation (co-IP) assay and Cycloheximide (CHX) chase assay

For Co-IP, pre-cleared protein from whole cell lysates were incubated with antibody against CASZ1 or RAF1 at 4 °C overnight, which was conjugated to AminoLink Plus Resin (Pierce, Rockford, IL), The IP targets were disassociated from the immobilized antibodies on the AminoLink Plus Resin by the gentle elution buffer. Eluted proteins were resolved using 10% SDS-PAGE, followed by western blot with appropriate antibodies. Cycloheximide (CHX) chase assay was used to determine the half-life of RAF1. CASZ1-interfered HCC cells were treated with CHX (25 μg/mL) for the indicated times, and then were harvested and analyzed by western blot as described above. RAF1 protein degradation rates were quantified by densitometry using time point zero as 100%.

Cell immunofluorescence staining

Indicated HCC cells (5 × 104 cells) were seeded into 6-well plate with glass coverslips for 24 h. Then cells were successively fixed in 4% paraformaldehyde, permeabilized with 0.2% Triton X-100, blocked with 1% BSA and incubated with primary antibody at 4 °C overnight. After washed with PBS, cells were incubated with appropriate DyLight-conjugated secondary antibody and DAPI (Vector laboratories, Burlingame, CA). Finally, the slides were mounted and images were captured using an inverted fluorescence microscope DMI4000-B (Leica).

HCC mouse models

Animal xenograft assays were conducted with 6-week-old male BALB/c nude mice (six mice per group). 5 × 106 indicated cells were subcutaneously injected into the right dorsal flank of nude mice. Tumor sizes were measured at the indicated time points and calculated with the following formula: Tumor volume = L × W2 × 0.5 (L, length; W, width) [28]. After 4 weeks, the mice were sacrificed, and the tumors were obtained to weigh and undergo further experiments. Orthotopic tumor implantation was performed as described previously [29]. Tumor formation and metastatic progression was monitored and quantified using the Xenogen IVIS imaging system 100 (Caliper Lifescience, Hopkinton, MA). After 8 weeks, the mice were sacrificed, and the livers and lungs were harvested, imaged and processed for histopathological examination. All animal experiments were approved by the Institutional Animal Care and Use Committee of Central South University.

Statistical analysis

Statistical analysis was performed using SPSS 18.0 software (SPSS Inc., Chicago, IL). The experimental data was presented as the mean ± SD and analyzed using Student’s t test or one-way ANOVA. The Chi-squared test was applied to examine the association between CASZ1 expression and clinical pathological parameters. Survival curves for patients were calculated using the Kaplan-Meier method and analyzed using the log-rank test. Prognostic factors were examined by univariate and multivariate analyses using the Cox proportional hazards model. Spearman’s rank analysis was performed to determine the correlation between different protein levels. All differences were deemed statistically significant at P < 0.05.

Results

CASZ1 is downregulated in human HCC tissues and cell lines

To determine the level of CASZ1 mRNA in HCC, qRT-PCR was performed in 15 normal liver tissues (NLs) and 50 pairs of HCC samples. Results showed that CASZ1 mRNA in HCC tissues was significantly lower than in the NLs (Fig. 1a), which was further verified by the analyses of mRNA sequencing datasets from Gene Expression Omnibus (Fig. 1b, GSE62232, GSE6764, GSE25097 and GSE64041, all P < 0.05). In addition, downregulation of CASZ1 (ANLT/HCC > 2) was detected in 34 of 50 (68%) HCCs compared to their matched adjacent non-tumor liver tissues (ANLTs) (Fig. 1c). Western blot analysis further confirmed CASZ1 expression was decreased in HCC tissues at protein level (Fig. 1d). Immunohistochemical analysis revealed that CASZ1 staining, mainly localized to the cytoplasm in the hepatic cells, was weaker in HCC tumor tissues than in their peri-tumor counterparts (Fig.1e). Moreover, we further detected the mRNA and protein levels of CASZ1 in eight HCC cell lines (MHCC97-H, SMMC7721, Huh7, HepG2, PLC/PRF/5, MHCC97-L, HCCLM3, Hep3B) and L02, an immortalized human liver cell line. Consistent with the above findings in HCC samples, our data showed that all examined HCC cell lines displayed lower mRNA and protein levels of CASZ1 than L02, especially for those (HCCLM3, HCC97-H, and Hep3B) with high invasion potential (Fig. 1f), which indicated a negative association between CASZ1 expression and HCC cell invasive ability. In summary, these results suggested that CASZ1 is downregulated in HCC, thus it may play an important role in HCC development.
Figure 1
Fig. 1

CASZ1 is downregulated in human HCC tissues and cell lines a. CASZ1 mRNA expression in 15 normal liver tissues (NLs) and 50 HCC tissues was analyzed by qRT-PCR. Data are shown as mean ± SD. ***P < 0.001. b CASZ1 expression was lower in HCC tissues than NLs according to the analysis of data from GEO (GSE62232, GSE6764, GSE25097, GSE64041, all P < 0.05). c Waterfall plot showing the downregulation of CASZ1 in 34 of 50 (68%) HCC samples compared to their matched adjacent non-tumor liver tissues (ANLTs). d The CASZ1 protein levels in HCCs, ANLTs and NLs were analyzed by Western blot. β-actin was used as a loading control. e Representative immunohistochemical images demonstrated CASZ1 protein was lowly expressed in HCC tumor tissues compared with their peri-tumor tissues. Magnification, × 100, × 400. f Expression of CASZ1 in HCC cell lines and L02, the normal liver cell line, were measured by qRT-PCR and western blot, respectively. *P < 0.05; **P < 0.01; ***P < 0.001 compared with L02

Low expression of CASZ1 is associated with aggressive clinicopathological characteristics and poor prognosis

To explore the clinical significance of CASZ1 expression in HCC, we scored the IHC staining of HCC clinical samples from two independent cohorts: the training cohort (n = 132) and the validation cohort (n = 100), and defined CASZ1 expression as low or high according to the scores mentioned in Methods. In these two cohorts, we found that the percentage of low CASZ1 was significantly higher in HCC tissues than in ANLTs (Fig. 2a). On clinicopathological correlation, CASZ1 expression was significantly associated with tumor size (P = 0.021), tumor nodule number (P = 0.033), capsulation formation (P < 0.001), Edmondson-Steiner grade (P = 0.005), BCLC stage (P = 0.027) and TNM stage (P = 0.020) in the training cohort, however, there was no statistical correlation between CASZ1 expression and other clinicopathologic parameters, such as sex, gender, microvascular invasion (MVI), macrovascular invasion (MAVI) and so on (P > 0.05) (Additional file 2: Table S2). Importantly, these findings were further confirmed in the validation cohort (Additional file 2: Table S2). Kaplan-Meier survival analysis in the training cohort showed that HCC patients with low CASZ1 had shorter OS (median OS: 19.0 v.s 48.0 months; P < 0.001) and DFS (median DFS: 15.7 v.s 37.0 months; P < 0.001) than those with high CASZ1 (Fig. 2b). In addition, multivariate analysis proved low CASZ1 as an independent risk factor for both OS (HR = 1.972; 95% CI: 1.154–3.369; P = 0.013) and DFS (HR = 2.259; 95% CI: 1.365–3.738; P = 0.002) in HCC patients (Fig. 2c and Additional file 2: Table S3). Consistent with these results, in the validation cohort, we also found that CASZ1 expression inversely correlated with poor OS and DFS, and served as an independent prognostic marker in HCC patients (Fig. 2d and Additional file 2: Table S4). Of note, when tumor recurrence was classified as early recurrence and late recurrence using 2 year as the cutoff, we observed that the prognostic significance of CASZ1 was existed in the early recurrence group (P < 0.001), but not in the late recurrence group (P = 0.079) (Fig. 2e), which was consistent with the results from validation cohort (Fig. 2f). Thus, low CASZ1 expression may be a predictor for HCC early recurrence. Taken together, the above findings indicated that CASZ1 is a potential prognostic marker for HCC patients, which may involve in HCC aggressiveness and metastasis.
Figure 2
Fig. 2

Low expression of CASZ1 is associated with aggressive clinicopathological characteristics and poor prognosis a. Representative images of low CASZ1 expression cases and high CASZ1 expression cases were shown (upper panel). Magnification, × 100, × 400. The percentages of low or high CASZ1 in paired HCC samples from the training and validation cohorts were compared (lower panel). b Kaplan-Meier analysis of OS and DFS based on CASZ1 expression in the training cohort. c Forest plots showing HR of OS and DFS for HCC patients in the indicated clinical subgroups of training cohort. d Kaplan-Meier analysis of OS and DFS based on CASZ1 expression in the validation cohort. e Kaplan-Meier analysis of early recurrence and late recurrence based on CASZ1 expression in the training cohort. f Kaplan-Meier analysis of early recurrence and late recurrence based on CASZ1 expression in the validation cohort

CASZ1 inhibits HCC cell proliferation, migration and invasion in vitro

To investigate the effects of CASZ1 on malignant phenotypes in HCC cells, we stably overexpressed CASZ1 in low CASZ1-expressing HCCLM3 cells, and knocked down it in high CASZ1-expressing PLC/PRF/5 cells using lentivirus transfection. The expression of CASZ1 in these resultant cells (HCCLM3CASZ1, HCCLM3Control, PLC/PRF/5shCASZ1 and PLC/PRF/5shCtr) were verified by qRT-PCR and western blot (Additional file 3: Figure S2A, B). Among the three shRNAs, we chose shRNA3, which achieved an 86% reduction in CASZ1 expression, for subsequent assays. Firstly, we analyzed the effects of CASZ1 on cell proliferation using MTT assay, which indicated that the cell proliferation rate was significantly decreased in HCCLM3CASZ1 group, but increased in PLC/PRF/5shCASZ1 group (Fig. 3a). Similarly, colony formation assay showed that overexpression of CASZ1 in HCCLM3 cells reduced the number of clones, whereas silencing CASZ1 in PLC/PRF/5 cells increased it (Fig. 3b). Next, we performed flow cytometry to investigate the effects of CASZ1 on cell cycle progression in HCC cells. As shown in Fig. 3c, overexpression of CASZ1 in HCCLM3 cells obviously increased the proportion of cells in G1 phase and decreased the proportion of cells in S phase, whereas knockdown of CASZ1 in PLC/PRF/5 cells resulted in the opposite trend, suggesting that CASZ1 may inhibit HCC cell proliferation by inducing cell cycle arrest at G1/S checkpoint. Furthermore, we investigated the potential role of CASZ1 in modulation of HCC cells to migrate and invade. In wound healing assay, we found that ectopic expression of CASZ1 decreased the rate of wound closure in HCCLM3 cells, whereas silencing CASZ1 in PLC/PRF/5 cells increased the rate of wound closure after scratch (Fig. 3d). Consistently, transwell invasion assays showed that HCCLM3CASZ1 group had less cells that passed through matrigel than HCCLM3Control group, while PLC/PRF/5shCASZ1 group had more invasive cells than PLC/PRF/5shCtr group (Fig. 3e). Collectively, these data strongly demonstrated that CASZ1 elicits a tumor-suppressive role in HCC progression by inhibiting cell proliferation, migration and invasion.
Figure 3
Fig. 3

CASZ1 inhibits HCC cell proliferation, migration and invasion in vitro a. The effects of CASZ1 on HCC cell proliferation was measured by MTT assay at different time points. b Representative imgages and quantification of cell clones in HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control groups, as determined by colony formation assay. c The effect of CASZ1 on HCC cell cycle progression was analyzed by flow cytometry. d Wound healing assay was performed to detect the migratory capacity of HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells. e Transwell invasion assay was performed to evaluate the invasive potential of CASZ1-interfered HCC cells. Each bar represents the mean ± SD of three independent experiments. *P < 0.05; **P < 0.01; ***P < 0.001

CASZ1 represses HCC growth and metastasis in vivo

To verify the capacity of CASZ1 to inhibit HCC progression in vivo, we established subcutaneous xenograft tumor models and orthotopic xenograft tumor models using luciferase-labelled HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells. Consistent with the in vitro results, CASZ1 overexpression in HCCLM3 cells significantly inhibited tumor growth, as evidenced by tumor sizes and weights, whereas knockdown of CASZ1 in PLC/PRF/5 cells markedly increased tumor burden in vivo (Fig. 4a, b). Moreover, in liver orthotopic xenograft tumor models, IVIS imaging showed that tumors in HCCLM3CASZ1 group had weaker fluorescence signals than those in HCCLM3control group, however, tumors from PLC/PRF/5shCASZ1 group exhibited stronger fluorescence signals than those from PLC/PRF/5shCtr group (Fig. 4c), which indicated that CASZ1 could inhibit HCC growth and metastasis in vivo. H&E staining of liver tumors further confirmed the inhibitory role of CASZ1 in HCC intrahepatic metastasis, because tumors in HCCLM3CASZ1 group often had expansive tumor growth fronts with less invasive borders, whereas tumors from PLC/PRF/5shCASZ1 group exhibited invasive growth fronts with irregular tumor borders and tumor microsatellites (Fig. 4d). Moreover, ex-vivo bioluminescent imaging showed the incidence of lung metastasis was decreased in HCCLM3CASZ1 group, but increased in PLC/PRF/5shCASZ1 group (Fig. 4e). Consistently, H&E staining confirmed that the number of pulmonary metastatic nodules was obviously decreased in HCCLM3CASZ1 group, but increased in PLC/PRF/5shCASZ1 group (P < 0.05, Fig. 4f). Together, these data provided strong evidence to support the tumor-suppressive function of CASZ1 in HCC growth and metastasis in vivo.
Figure 4
Fig. 4

CASZ1 represses HCC growth and metastasis in vivo a. Effects of CASZ1 on HCC growth in subcutaneous xenograft model. The size of tumors was measured at indicated time points, and is shown as mean ± SD. **P < 0.01; ***P < 0.001. b Tumors were excised and weighted after mice were sacrificed. **P < 0.01. c Representative bioluminescent images of the orthotopic HCC model in HCCLM3Control, HCCLM3CASZ1, PLC/PRF/5shCtr and PLC/PRF/5shCASZ1 groups (n = 6 for each group, left panel). The colored region represents the fluorescence signal of HCC cells in nude mice. Luciferase activity was quantified for experimental and control groups (right panel). **P < 0.01. d Representative H&E-stained sections of orthotopic primary liver tumors formed by HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells (original magnified × 100; inserted figures magnified × 400). e The presence of lung metastasis was examined in ex vivo bioluminescence imaging. f Representative H&E staining of pulmonary metastatic nodules in experimental and control groups (left panel: original magnified × 100; inserted figures magnified × 400). The number of lung metastatic nodules in each group is presented as mean ± SD (right panel). *P < 0.05; **P < 0.01

CASZ1 inhibits HCC growth and metastasis via inactivating the MAPK/ERK signaling

To probe the molecular mechanism underlying CASZ1-mediated inhibition of HCC growth and metastasis, we performed a Cignal Finder Cancer 10-Pathway Reporter Array in CASZ1 overexpression or knockdown HCC cells. Results showed that MAPK/ERK signaling pathway was the most significantly altered pathway when CASZ1 was interfered in HCC cells (Fig. 5a), indicating that CASZ1 may function via regulating the MAPK/ERK signaling. As expected, western blot analysis revealed that CASZ1 overexpression inhibited the phosphorylation of ERK in HCCLM3 cells, whereas CASZ1 knockdown resulted in an increase of p-ERK in PLC/PRF/5 cells, however, the total level of ERK kept unchanged (Fig. 5b). We further investigated the effect of CASZ1 on the expression of several genes related to cancer cell proliferation and invasion, such as MMP2, MMP9, cyclinD1 and epithelial-mesenchymal transition (EMT) genes, which were controlled by the MAPK/ERK pathway [3032]. Data showed that the protein levels of MMP2, MMP9 and cyclinD1 were greatly decreased in CASZ1-ovexpressed HCCLM3 cells but increased in CASZ1-silenced PLC/PRF/5 cells (Fig. 5b). However, CASZ1 exhibited no significant effect on EMT gene expression and cell morphological change in HCC cells (Additional file 4: Figure S3A, B). IHC staining further demonstrated that the expression of p-ERK, MMP2, MMP9 and cyclinD1 were decreased in tumors induced by HCCLM3CASZ1 cells, whereas increased in tumors induced by PLC/PRF/5shCASZ1 cells (Additional file 4: Figure S3C). Moreover, we treated CASZ1-interfered HCC cells with U0126, a highly selective MEK inhibitor, and found that U0126 could obviously attenuated the promoting effect of low CASZ1 on the levels of p-ERK, MMP2, MMP9 and cyclinD1 in HCCLM3Control and PLC/PRF/5shCASZ1 cells (Fig. 5c). But due to the low level of phosphorylated ERK in the high CASZ1-expressing cells, further inhibition of ERK activity by U0126 didn’t affect the expression of p-ERK, MMP2, MMP9 and cyclinD1 in HCCLM3CASZ1 and PLC/PRF/5shCtr cells (Fig. 5c). Similarly, MTT, wound healing and transwell invasion assays also showed that U0126 markedly reduced the proliferative, migrative and invasive abilities of HCCLM3Control and PLC/PRF/5shCASZ1cells, but produced no significant effects in high CASZ1-expressing cells (Fig. 5d-f). Together, these data indicated that CASZ1 could negatively regulate MAPK/ERK signaling and its downstream effectors to inhibit HCC progression.
Figure 5
Fig. 5

CASZ1 inhibits HCC growth and metastasis via inactivating the MAPK/ERK signaling a. 10-Pathway Reporter Array was performed to detect the signaling changes in CASZ1-interfered HCC cells. **P < 0.01. b The expression of critical members and downstream effectors of MAPK/ERK pathway was examined by western blot in HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells. c The levels of p-ERK, MMP2, MMP9 and cyclinD1 were determined by western blot in HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells treated with U0126 (10 μM) or DMSO control. d-f. HCCLM3CASZ1, PLC/PRF/5shCASZ1 and their control cells were treated with U0126 (10 μM) or DMSO control and then subjected to MTT (d), wound healing (e) and transwell invasion (f) assays

CASZ1 decreases RAF1 expression by reducing the protein stability of RAF1

To explore the molecular mechanism by which CASZ1 exerted its tumor-suppressive function in HCC cells, we reviewed literatures and searched BioGrid 3.4 database (Additional file 5: Figure S4A). We found that CASZ1 might interact with RAF1, a highly-conserved serine/threonine kinase of the MAPK pathway that involved in cell proliferation, transformation, survival and metastasis of various cancers [3335]. As expected, immunofluorescence staining results showed that CASZ1 co-localized with RAF1 in the cytoplasm of CASZ1-transfected HCCLM3 cells (Fig. 6a), while co-IP results revealed CASZ1 and RAF1 could interact with each other in HCC cells (Fig. 6b). Next, we investigated whether the interaction between CASZ1 and RAF1 could affect RAF1 expression in HCC cells. Interestingly, we found that ectopic expression of CASZ1 in HCCLM3 cells decreased the protein level of RAF1, whereas silencing CASZ1 in PLC/PRF/5 cells increased RAF1 protein expression (Fig. 6c), however, manipulating CASZ1 expression had little effect on RAF1 mRNA expression (Additional file 5: Figure S4B). The above results indicated that CASZ1 downregulates RAF1 at the protein (but not mRNA) level. Moreover, IHC staining in 50 HCC samples randomly selected from the training and validation cohorts showed that RAF1 protein was highly expressed in HCC tissues and negatively correlated with CASZ1 expression (P < 0.001, r = − 0.643, Fig. 6d). Subsequently, we investigated whether CASZ1 decreased RAF1 level in HCC cells by regulating its protein stability. As shown in Fig. 6e, overexpression of CASZ1 could dramatically decreased the half-life of RAF1 protein after added translation inhibitor cycloheximide (CHX). Conversely, silence of CASZ1 remarkably prolong the half-life of RAF1 protein (Fig. 6e). Furthermore, MG132, the proteasome inhibitor, rescued the decrease of RAF1 induced by CASZ1 overexpression in HCCLM3 cells (Fig. 6f). These results indicated that CASZ1 decreases RAF1 expression in HCC cells by reducing the protein stability of RAF1.
Figure 6
Fig. 6

CASZ1 decreases RAF1 expression by reducing the protein stability of RAF1 a. HCCLM3 cells transfected with CASZ1 were fixed for the double immunofluorescence staining, and colocalization of CASZ1 with RAF1 were visualized as yellow fluorescence in merge panel. Scale bar, 25 μm. b Co-immunoprecipitation assay was performed to analyze the direct binding between CASZ1 and RAF1 in HCCLM3CASZ1, HCCLM3 and PLC/PRF/5 cells. c The expression of RAF1 was determined in CASZ1-interfered HCC cells by western blot. d Correlation between CASZ1 and RAF1 was measured in 50 HCC samples. Representative IHC staining of CASZ1 and RAF1 (left panel, magnification, × 400) in serial sections are shown, indicating a negative correlation between the protein level of CASZ1 and RAF1 in the clinical samples (r = − 0.643, P < 0.001, right panel). e The half-life of RAF1 protein in HCC cells was analyzed following treatment with cycloheximide (CHX, 25 μg/ml) for the indicated time points. The half-life of RAF1 protein was decreased in HCCLM3 cells with CASZ1 overexpression, but increased in PLC/PRF/5 cells with CASZ1 knockdown. f MG-132 (20 μM) was used to inhibit the proteasomal degradation in HCCLM3 cells. MG-132 treatment reversed the downregulation of RAF1 protein induced by CASZ1 overexpression. *** P < 0.001

RAF1 is critical for CASZ1-mediated inhibition of MAPK/ERK signaling and HCC progression

To test whether RAF1 is indispensable for CASZ1 to inactivate the MAPK/ERK signaling and inhibit HCC progression, we transfected the RAF1 ectopic expression plasmid into HCCLM3CASZ1 cells, and RAF1-shRNA into PLC/PRF5shCASZ1 cells. The ectopic expression and silence efficacy of RAF1 was varified by qRT-PCR and western blot, respectively (Additional file 6: Figure S5A, B). We found that the suppressive effect of CASZ1 on the levels of p-ERK, MMP2, MMP9 and cyclinD1 was significantly abrogated by RAF1 overexpression in HCCLM3CASZ1 cells, while the promotion effect of CASZ1 silence on these proteins expression was greatly inhibited by RAF1 knockdown in PLC/PRF/5shCASZ1 cells, however, altering RAF1 expression didn’t affect CASZ1 levels in HCC cells (Fig. 7a). These data indicated that RAF1 is necessary for the inactivation of MAPK/ERK signaling by CASZ1. Furthermore, the RAF1-dependency on CASZ1-mediated inhibition of HCC progression was also assessed by gain-and-loss function assays, which showed that overexpression of RAF1 in HCCLM3CASZ1 cells restored their proliferation and metastatic capacity, whereas knockdown of RAF1 in PLC/PRF/5shCASZ1 cells eliminated the promoting effect of CASZ1 silence on cell proliferation, migration and invasion (Fig. 7b-d and Additional file 6: Figure S5C). Together, these results proved that CASZ1 inhibits HCC growth and metastasis by regulating MAPK/ERK signaling via RAF1 in HCC cells (Fig. 7e).
Figure 7
Fig. 7

RAF1 is critical for CASZ1-mediated inhibition of MAPK/ERK signaling and HCC progression a. Western blot analysis of CASZ1, RAF1, p-ERK, MMP2, MMP9 and cyclinD1 expression in CASZ1-interfered HCC cells with RAF1 knockdown or ectopic expression. b-d. MTT (b), wound healing (c) and transwell invasion (d) assays were performed to test the influence of RAF1 on the proliferation, migration and invasion abilities of CASZ1-interfered HCC cells with RAF1 knockdown or ectopic expression. e Schematic depiction of the mechanism underlying CASZ1-mediated inhibition of HCC cell proliferation, migration and invasion based on our study

Discussion

Human CASZ1 gene is mapped on chromosome 1p36 and has a central role in diverse biological processes, such as neurogenesis, cardiac development and vascular morphogenesis [36]. Previous studies have reported the controversial roles of CASZ1 in several cancers [20, 22], which may be related to tumor and tissue specificity. However, to date, the relationship between CASZ1 and HCC progression is still unclear. In the present study, we proved that CASZ1 expression was obviously decreased in HCC tissues and cell lines. Overexpression of CASZ1 markedly inhibited HCC cell proliferation, migration and invasion in vitro, whereas knockdown of CASZ1 exerted the opposing effects. Interestingly, cell cycle analysis by flow cytometry showed that CASZ1 could induce cell cycle arrested at G1/S checkpoint. Furthermore, the in vivo animal experiments demonstrated that CASZ1 overexpression not only inhibits tumor growth, but also suppresses HCC metastasis, as determined by IVIS detection and H&E staining. Previous studies indicated that CASZ1 is a metastatic promoter in ovarian cancer [22], however, Liu et al. proved CASZ1 inhibits cell proliferation and migration in neuroblastoma [20, 21]. In the present study, our findings were in accordance with Liu’s report, and strongly demonstrated that CASZ1 is a tumor suppressor in HCC, which may be a potential therapeutic target for HCC.

In this study, we further explored the clinical significance of CASZ1 in two independent study cohorts consisting of 232 HCC subjects. We found that low CASZ1 significantly correlated with aggressive clinicopathologic features, such as larger tumor size, multiple tumor nodules, lack of capsule, higher Edmondson-Steiner grade, advanced BCLC stage and TNM stage, which further proved the suppressive role of CASZ1 in HCC progression. Moreover, survival analysis revealed that CASZ1 is an independent predictor for HCC prognosis, and low CASZ1 always indicated a shorter OS and DFS for HCC patients. Notably, we also observed that HCC patients in the low CASZ1 group had a significantly higher early recurrence rate than those from the high CASZ1 group, which suggested a potential predictive role of CASZ1 in HCC early recurrence. It’s well known that early recurrence is an important adverse prognostic factor, which mainly results from dissemination of metastatic HCC cells [37, 38], thus detecting CASZ1 expression may help to predict HCC progression, and direct personalize therapy for HCC patients in the future. To the best of our knowledge, this is the first report detailing CASZ1 as a prognostic predictor in HCC.

We then explored the molecular mechanism of CASZ1 to inhibit HCC progression. Although CASZ1 was reported to modulate EGFL7/RhoA pathway and pRb activity in different cell types [16, 39], however, given the context-dependent function of CASZ1 in various cancers, we speculated that CASZ1 may have a different mechanism to counteract HCC growth and metastasis. Indeed, the results of 10-Pathway Reporter Array in CASZ1-interfered HCC cells showed that CASZ1 could significantly inhibited the activity of MAPK/ERK signaling, which was further confirmed by western blot and IHC assays. Our data also revealed that CASZ1 significantly reduced the levels of MMP2, MMP9 and cyclinD1 in HCCLM3CASZ1 cells, but increased their expression in PLC/PRF/5shCASZ1 cells. As the downstream effectors of p-ERK, MMP2 and MMP9 are important for tumor invasion and metastasis by degrading basement membrane components [40], while cyclinD1 acts on G1-S progression of the cell cycle [41], thus they may decipher the function of CASZ1 in HCC proliferation and metastasis. Interestingly, although CASZ1 was reported to promote cell migration and invasion via EMT in ovarian cancer [22], however, in this study, we found that altering CASZ1 expression in HCC cells had no significant effects on the EMT gene expression and cell morphologic changes, indicating the role of CASZ1 in HCC progression was EMT-independent. To further examine whether the tumor-suppressive effects of CASZ1 were dependent on MAPK/ERK pathway, we treated CASZ1-interfered HCC cells with a MEK inhibitor U0126. Data showed that U0126 could effectively decrease the expression of p-ERK, MMP2, MMP9 and cyclinD1 in low CASZ1-expressing HCC cells. Moreover, it also abolished low CASZ1-induced proliferative, migratory and invasive ability in HCCLM3Control and PLC/PRF/5shCASZ1 cells. Taken together, the above findings indicated that CASZ1 inhibits HCC progression via inactivating the MAPK/ERK signaling.

RAF1 is an important kinase that transduces signals from the cell membrane to nucleus and activates MAPK/ERK pathway [42]. Accumulating evidences indicate that RAF1 is highly expressed in various malignant tumors, including HCC [35, 43, 44]. Moreover, Chen et al. reported that increased RAF1 in HCC is significantly correlated with poor prognosis [45]. In this study, we demonstrated that RAF1 was negatively regulated by CASZ1 in HCC cells, and there is an inverse correlation between CASZ1 and RAF1 protein levels in HCC clinical specimens. Importantly, we also proved that CASZ1 could interact with RAF1 and attenuate RAF1 expression by regulating its protein stability in HCC cells, however, the exact mechanism for CASZ1-mediated protein degradation of RAF1 requires further investigation in the future. Moreover, we found that CASZ1-induced RAF1 downregulation contributed to the inhibitory effects of CASZ1 on the MAPK/ERK signaling and HCC progression. Because ectopic expression of RAF1 effectively impeded the ability of CASZ1 to inactivate MAPK/ERK signaling and inhibit cell proliferation, migration and invasion in HCCLM3 cells, whereas silencing RAF1 offset these promoting effects of CASZ1 knockdown in PLC/PRF/5 cells. Thus, our study provided evidence to support that CASZ1 exerts its inhibitory function in HCC progression through regulating MAPK/ERK pathway via RAF1.

Conclusions

In summary, we proved that CASZ1 expression is downregulated in HCC tissues, which significantly correlated with aggressive clinicopathological characteristics, poor prognosis and early recurrence of HCC patients. Furthermore, CASZ1 inhibits HCC cell proliferation, migration and invasion through regulating MAPK/ERK signaling via RAF1. Thus these findings together defined CASZ1 as a tumor suppressor in HCC, which may be a novel prognostic biomarker and therapeutic target for HCC patients.

Abbreviations

AFP: 

alpha-fetoprotein

ANLT: 

adjacent non-tumor liver tissue

BCLC: 

Barcelona Clinic Liver Cancer

CASZ1: 

castor zinc finger 1

DFS: 

disease-free survival

ERK: 

extracellular signal-regulated kinase

GAPDH: 

glyceraldehyde-3-phosphate dehydrogenase

H&E: 

hematoxylin and eosin

HCC: 

hepatocellular carcinoma

IHC: 

immunohistochemistry

MAPK: 

mitogen-activated protein kinase

MAVI: 

macrovascular invasion

MMP: 

matrix metalloproteinase

MVI: 

microvascular invasion

OS: 

overall survival

RAF1: 

raf-1 proto-oncogene, serine/threonine kinase

shRNA: 

short-hairpin RNA

TNM: 

tumor-node-metastasis

Declarations

Acknowledgements

Not applicable

Funding

This work was supported by National Natural Science Foundation of China (81172018, 81272395), Key Project of National Natural Science Foundation of China (81330057), National Key R&D Program of China (2016YFC0902400), Specialized Research Fund for Doctoral Program of Higher Education of China (20130162130007), Fundamental Research Funds for the Central Universities of Central South University (2014zzts088) and Key Project of Science & Technology Plan of Science & Technology Department of Hunan Province (2014CK2003).

Authors’ contributions

WJL, YMY and XS conceived the study and wrote the manuscript; WJL, YMY and SB conducted the experiments and contributed to the analysis of data. XS, SB and LYM collected clinical samples and corresponding clinical data. YLY and XS revised the manuscript. All authors read and approved the final manuscript.

Ethics approval and consent to participate

The studies were approved by the Ethics Committee of Xiangya Hospital of Central South University and Affiliated Cancer Hospital of Xiangya School of Medicine. Written informed consent was obtained from all patients. Animal experiments were approved by the Institutional Animal Care and Use Committee of Central South University.

Consent for publication

Not applicable

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

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Authors’ Affiliations

(1)
Liver Cancer Laboratory, Department of Surgery, Xiangya Hospital, Central South University, Changsha, China
(2)
Department of Obstetrics and Gynecology, The Second Xiangya Hospital of Central South University, Changsha, China
(3)
Department of Surgery, Xiangya Hospital, Central South University, Changsha, China

References

  1. Chen W, Zheng R, Baade PD, Zhang S, Zeng H, Bray F, Jemal A, Yu XQ, He J. Cancer statistics in China, 2015. CA Cancer J Clin. 2016;66:115–32.View ArticlePubMedGoogle Scholar
  2. Torre LA, Bray F, Siegel RL, Ferlay J, Lortet-Tieulent J, Jemal A. Global cancer statistics, 2012. CA Cancer J Clin. 2015;65:87–108.View ArticlePubMedGoogle Scholar
  3. Forner A, Llovet JM, Bruix J. Hepatocellular carcinoma. Lancet. 2012;379:1245–55.View ArticlePubMedGoogle Scholar
  4. El-Serag HB. Hepatocellular carcinoma. N Engl J Med. 2011;365:1118–27.View ArticlePubMedGoogle Scholar
  5. Xia L, Huang W, Tian D, Zhu H, Qi X, Chen Z, Zhang Y, Hu H, Fan D, Nie Y, Wu K. Overexpression of forkhead box C1 promotes tumor metastasis and indicates poor prognosis in hepatocellular carcinoma. Hepatology. 2013;57:610–24.View ArticlePubMedGoogle Scholar
  6. Ye QH, Zhu WW, Zhang JB, Qin Y, Lu M, Lin GL, Guo L, Zhang B, Lin ZH, Roessler S, et al. GOLM1 modulates EGFR/RTK cell-surface recycling to drive hepatocellular carcinoma metastasis. Cancer Cell. 2016;30:444–58.View ArticlePubMedPubMed CentralGoogle Scholar
  7. Hou G, Chen L, Liu G, Li L, Yang Y, Yan HX, Zhang HL, Tang J, Yang YC, Lin X, et al. Aldehyde dehydrogenase-2 (ALDH2) opposes hepatocellular carcinoma progression by regulating AMP-activated protein kinase signaling in mice. Hepatology. 2017;65:1628–44.View ArticlePubMedGoogle Scholar
  8. Mellerick DM, Kassis JA, Zhang SD, Odenwald WF. Castor encodes a novel zinc finger protein required for the development of a subset of CNS neurons in drosophila. Neuron. 1992;9:789–803.View ArticlePubMedGoogle Scholar
  9. Cui X, Doe CQ. Ming is expressed in neuroblast sublineages and regulates gene expression in the drosophila central nervous system. Development. 1992;116:943–52.PubMedGoogle Scholar
  10. Hitier R, Chaminade M, Preat T. The Drosophila Castor gene is involved in postembryonic brain development. Mech Dev. 2001;103:3–11.View ArticlePubMedGoogle Scholar
  11. Vacalla CM, Theil T. Cst, a novel mouse gene related to drosophila Castor, exhibits dynamic expression patterns during neurogenesis and heart development. Mech Dev. 2002;118:265–8.View ArticlePubMedGoogle Scholar
  12. Liu Z, Yang X, Tan F, Cullion K, Thiele CJ. Molecular cloning and characterization of human Castor, a novel human gene upregulated during cell differentiation. Biochem Biophys Res Commun. 2006;344:834–44.View ArticlePubMedGoogle Scholar
  13. Christine KS, Conlon FL. Vertebrate CASTOR is required for differentiation of cardiac precursor cells at the ventral midline. Dev Cell. 2008;14:616–23.View ArticlePubMedPubMed CentralGoogle Scholar
  14. Liu Z, Li W, Ma X, Ding N, Spallotta F, Southon E, Tessarollo L, Gaetano C, Mukouyama YS, Thiele CJ. Essential role of the zinc finger transcription factor Casz1 for mammalian cardiac morphogenesis and development. J Biol Chem. 2014;289:29801–16.View ArticlePubMedPubMed CentralGoogle Scholar
  15. Amin NM, Gibbs D, Conlon FL. Differential regulation of CASZ1 protein expression during cardiac and skeletal muscle development. Dev Dyn. 2014;243:948–56.View ArticlePubMedPubMed CentralGoogle Scholar
  16. Charpentier MS, Christine KS, Amin NM, Dorr KM, Kushner EJ, Bautch VL, Taylor JM, Conlon FL. CASZ1 promotes vascular assembly and morphogenesis through the direct regulation of an EGFL7/RhoA-mediated pathway. Dev Cell. 2013;25:132–43.View ArticlePubMedPubMed CentralGoogle Scholar
  17. Charpentier MS, Taylor JM, Conlon FL. The CASZ1/Egfl7 transcriptional pathway is required for RhoA expression in vascular endothelial cells. Small GTPases. 2013;4:231–5.View ArticlePubMedPubMed CentralGoogle Scholar
  18. Hoff AM, Johannessen B, Alagaratnam S, Zhao S, Nome T, Lovf M, Bakken AC, Hektoen M, Sveen A, Lothe RA, Skotheim RI. Novel RNA variants in colorectal cancers. Oncotarget. 2015;6:36587–602.View ArticlePubMedPubMed CentralGoogle Scholar
  19. Kekeeva T, Tanas A, Kanygina A, Alexeev D, Shikeeva A, Zavalishina L, Andreeva Y, Frank GA, Zaletaev D. Novel fusion transcripts in bladder cancer identified by RNA-seq. Cancer Lett. 2016;374:224–8.View ArticlePubMedGoogle Scholar
  20. Liu Z, Yang X, Li Z, McMahon C, Sizer C, Barenboim-Stapleton L, Bliskovsky V, Mock B, Ried T, London WB, et al. CASZ1, a candidate tumor-suppressor gene, suppresses neuroblastoma tumor growth through reprogramming gene expression. Cell Death Differ. 2011;18:1174–83.View ArticlePubMedPubMed CentralGoogle Scholar
  21. Liu Z, Naranjo A, Thiele CJ. CASZ1b, the short isoform of CASZ1 gene, coexpresses with CASZ1a during neurogenesis and suppresses neuroblastoma cell growth. PLoS One. 2011;6:e18557.View ArticlePubMedPubMed CentralGoogle Scholar
  22. Wu YY, Chang CL, Chuang YJ, Wu JE, Tung CH, Chen YC, Chen YL, Hong TM, Hsu KF. CASZ1 is a novel promoter of metastasis in ovarian cancer. Am J Cancer Res. 2016;6:1253–70.PubMedPubMed CentralGoogle Scholar
  23. Altman DG, McShane LM, Sauerbrei W, Taube SE. Reporting recommendations for tumor marker prognostic studies (REMARK): explanation and elaboration. PLoS Med. 2012;9:e1001216.View ArticlePubMedPubMed CentralGoogle Scholar
  24. Xiao S, Chang RM, Yang MY, Lei X, Liu X, Gao WB, Xiao JL, Yang LY. Actin-like 6A predicts poor prognosis of hepatocellular carcinoma and promotes metastasis and epithelial-mesenchymal transition. Hepatology. 2016;63:1256–71.View ArticlePubMedPubMed CentralGoogle Scholar
  25. Liu L, Dai Y, Chen J, Zeng T, Li Y, Chen L, Zhu YH, Li J, Li Y, Ma S, et al. Maelstrom promotes hepatocellular carcinoma metastasis by inducing epithelial-mesenchymal transition by way of Akt/GSK-3beta/snail signaling. Hepatology. 2014;59:531–43.View ArticlePubMedGoogle Scholar
  26. Qu K, Xu X, Liu C, Wu Q, Wei J, Meng F, Zhou L, Wang Z, Lei L, Liu P. Negative regulation of transcription factor FoxM1 by p53 enhances oxaliplatin-induced senescence in hepatocellular carcinoma. Cancer Lett. 2013;331:105–14.View ArticlePubMedGoogle Scholar
  27. Pullar CE, Chen J, Isseroff RR. PP2A activation by beta2-adrenergic receptor agonists: novel regulatory mechanism of keratinocyte migration. J Biol Chem. 2003;278:22555–62.View ArticlePubMedGoogle Scholar
  28. Wang YP, Yu GR, Lee MJ, Lee SY, Chu IS, Leem SH, Kim DG. Lipocalin-2 negatively modulates the epithelial-to-mesenchymal transition in hepatocellular carcinoma through the epidermal growth factor (TGF-beta1)/Lcn2/Twist1 pathway. Hepatology. 2013;58:1349–61.View ArticlePubMedGoogle Scholar
  29. Chang RM, Yang H, Fang F, Xu JF, Yang LY. MicroRNA-331-3p promotes proliferation and metastasis of hepatocellular carcinoma by targeting PH domain and leucine-rich repeat protein phosphatase. Hepatology. 2014;60:1251–63.View ArticlePubMedGoogle Scholar
  30. Song H, Li Y, Lee J, Schwartz AL, Bu G. Low-density lipoprotein receptor-related protein 1 promotes cancer cell migration and invasion by inducing the expression of matrix metalloproteinases 2 and 9. Cancer Res. 2009;69:879–86.View ArticlePubMedPubMed CentralGoogle Scholar
  31. Hu X, Zhai Y, Kong P, Cui H, Yan T, Yang J, Qian Y, Ma Y, Wang F, Li H, et al. FAT1 prevents epithelial mesenchymal transition (EMT) via MAPK/ERK signaling pathway in esophageal squamous cell cancer. Cancer Lett. 2017;397:83–93.View ArticlePubMedGoogle Scholar
  32. Peng H, Dara L, Li TW, Zheng Y, Yang H, Tomasi ML, Tomasi I, Giordano P, Mato JM, Lu SC. MAT2B-GIT1 interplay activates MEK1/ERK 1 and 2 to induce growth in human liver and colon cancer. Hepatology. 2013;57:2299–313.View ArticlePubMedPubMed CentralGoogle Scholar
  33. Karreth FA, Frese KK, DeNicola GM, Baccarini M, Tuveson DA. C-Raf is required for the initiation of lung cancer by K-Ras (G12D). Cancer Discov. 2011;1:128–36.View ArticlePubMedPubMed CentralGoogle Scholar
  34. Ehrenreiter K, Kern F, Velamoor V, Meissl K, Galabova-Kovacs G, Sibilia M, Baccarini M. Raf-1 addiction in Ras-induced skin carcinogenesis. Cancer Cell. 2009;16:149–60.View ArticlePubMedGoogle Scholar
  35. Hwang YH, Choi JY, Kim S, Chung ES, Kim T, Koh SS, Lee B, Bae SH, Kim J, Park YM. Over-expression of c-raf-1 proto-oncogene in liver cirrhosis and hepatocellular carcinoma. Hepatol Res. 2004;29:113–21.View ArticlePubMedGoogle Scholar
  36. Henrich KO, Schwab M, Westermann F. 1p36 tumor suppression--a matter of dosage? Cancer Res. 2012;72:6079–88.View ArticlePubMedGoogle Scholar
  37. Portolani N, Coniglio A, Ghidoni S, Giovanelli M, Benetti A, Tiberio GA, Giulini SM. Early and late recurrence after liver resection for hepatocellular carcinoma: prognostic and therapeutic implications. Ann Surg. 2006;243:229–35.View ArticlePubMedPubMed CentralGoogle Scholar
  38. Liu Y, Zhang JB, Qin Y, Wang W, Wei L, Teng Y, Guo L, Zhang B, Lin Z, Liu J, et al. PROX1 promotes hepatocellular carcinoma metastasis by way of up-regulating hypoxia-inducible factor 1alpha expression and protein stability. Hepatology. 2013;58:692–705.View ArticlePubMedGoogle Scholar
  39. Liu Z, Rader J, He S, Phung T, Thiele CJ. CASZ1 inhibits cell cycle progression in neuroblastoma by restoring pRb activity. Cell Cycle. 2013;12:2210–8.View ArticlePubMedPubMed CentralGoogle Scholar
  40. Dhillon AS, Hagan S, Rath O, Kolch W. MAP kinase signalling pathways in cancer. Oncogene. 2007;26:3279–90.View ArticlePubMedGoogle Scholar
  41. Torii S, Yamamoto T, Tsuchiya Y, Nishida E. ERK MAP kinase in G cell cycle progression and cancer. Cancer Sci. 2006;97:697–702.View ArticlePubMedGoogle Scholar
  42. Wellbrock C, Karasarides M, Marais R. The RAF proteins take centre stage. Nat Rev Mol Cell Biol. 2004;5:875–85.View ArticlePubMedGoogle Scholar
  43. Wang F, Jiang C, Sun Q, Yan F, Wang L, Fu Z, Liu T, Hu F. miR-195 is a key regulator of Raf1 in thyroid cancer. Onco Targets Ther. 2015;8:3021–8.View ArticlePubMedPubMed CentralGoogle Scholar
  44. Chang CJ, Yang JY, Xia W, Chen CT, Xie X, Chao CH, Woodward WA, Hsu JM, Hortobagyi GN, Hung MC. EZH2 promotes expansion of breast tumor initiating cells through activation of RAF1-beta-catenin signaling. Cancer Cell. 2011;19:86–100.View ArticlePubMedPubMed CentralGoogle Scholar
  45. Chen L, Shi Y, Jiang CY, Wei LX, Wang YL, Dai GH. Expression and prognostic role of pan-Ras, Raf-1, pMEK1 and pERK1/2 in patients with hepatocellular carcinoma. Eur J Surg Oncol. 2011;37:513–20.View ArticlePubMedGoogle Scholar

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© The Author(s). 2018

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