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. 2015 Jun 23;5:10466. doi: 10.1038/srep10466

Prognostic significance of kynurenine 3-monooxygenase and effects on proliferation, migration, and invasion of human hepatocellular carcinoma

Haojie Jin 1,*, Yurong Zhang 1,*, Haiyan You 1,*, Xuemei Tao 1, Cun Wang 1, Guangzhi Jin 2, Ning Wang 1, Haoyu Ruan 1, Dishui Gu 1, Xisong Huo 1, Wenming Cong 2,a, Wenxin Qin 1,b
PMCID: PMC4479133  PMID: 26099564

Abstract

Kynurenine 3-monooxygenase (KMO) is a pivotal enzyme in the kynurenine pathway of tryptophan degradation and plays a critical role in Huntington’s and Alzheimer’s diseases. This study aimed to examine the expression of KMO in human hepatocellular carcinoma (HCC) and investigate the relationship between its expression and prognosis of HCC patients. We first analyzed KMO expression in 120 paired HCC samples (HCC tissues vs matched adjacent non-cancerous liver tissues), and 205 clinical HCC specimens using immunohistochemistry (IHC). Kaplan-Meier survival and Cox regression analyses were executed to evaluate the prognosis of HCC. The results of IHC analysis showed that KMO expression was significantly higher in HCC tissues than that in normal liver tissues (all p < 0.05). Survival and recurrence analyses showed that KMO was an independent prognostic factor for overall survival (OS) and time to recurrence (TTR) (both p<0.01). And in vitro studies revealed that KMO positively regulated proliferation, migration, and invasion of HCC cells. These results suggest that KMO exhibits tumor-promoting effects towards HCC and it may serve as a novel prognostic marker in HCC.

Hepatocellular carcinoma (HCC) is the fifth most prevalent cancer and the third major cause of cancer-related death in the world1. Despite many advances in HCC therapy such as surgery, chemotherapy and biologics, majority of HCC patients still has a poor prognosis due to high frequency of metastasis and recurrence2,3. It has been reported that the 5-year survival rate of HCC patients is as low as 25–39%, and its recurrence rate remains about 80%4,5. Therefore, it is critical to understand the etiology, illustrate the mechanisms underlying HCC initiation and progression, and further identify valuable factors for prognosis prediction and novel therapeutic strategies.

Kynurenine 3-monooxygenase (KMO), a pivotal enzyme in the kynurenine pathway (KP) of tryptophan degradation, has been suggested to play a critical role in Huntington’s (HD) and Alzheimer’s diseases (AD)6,7,8. It is widely distributed in peripheral tissues, including liver and kidney, and in phagocytes such as macrophages and monocytes9,10, and also in microglial cells in central nervous system11,12. As a FAD-dependent enzyme, KMO localizes to the outer mitochondrial membrane and controls the synthesis of several KP metabolites, including 3-hydroxykynurenine (3-HK), quinolinic acid (QUIN), and kynurenicacid (KYNA), as well as anthranilic acid. These bioactive metabolites were found to frequently associate with brain disorders8, peripheral inflammatory conditions13, and cancer14,15. However, whether KMO deregulation also occurs in human HCC remains unclear. In this study, we investigated the expression of KMO, evaluated its prognostic significance, and explored the role of KMO in HCC. Our data indicate that KMO is remarkably increased in HCC and can be served as a promising biomarker of HCC prognosis.

Materials and Methods

Patients and Specimens

Paraffin-embedded pathological specimens in prognostic groups were obtained from the archives of the Eastern Hepatobiliary Hospital (EHBH) between 1996 and 2001, and followed until October 2010. No patients in this study received sorafenib treatment. Tumor stage was defined according to the American Joint Committee on Cancer (AJCC 2010, 7th edition) TNM staging system16. The grade of tumor differentiation was assigned by the Edmondson-Steiner grading system. Micrometastases were defined as tumors adjacent to the border of the main tumor that was only observed under the microscope17. Then, 205 and 182 HCC patients were randomly selected from this cohort as the study population and reviewed retrospectively.

Patient follow-up was performed every 2–3 months during the first year after surgery and 3–6 months thereafter until October 2010. The median follow-up was 40.8 month (range, 0.3–141 month). All follow-up examinations were performed by two physicians unaware of the study. All patients were monitored by abdomen ultrasonography, chest X-ray, and a test for the serum AFP concentration every month during the first year after surgery and every 3–6 months thereafter. A computed tomography scan or magnetic resonance imaging of the abdomen was performed every 6 months or immediately after a recurrence was suspected. The diagnosis criteria for recurrence were equal to that for the preoperative diagnosis. The overall survival (OS) was defined as the length of time between the surgery and death or the last follow-up examination. The time to recurrence (TTR) was calculated from the date of tumor resection until the detection of tumor recurrence, death or the last observation.

An additional 50 HCC patients as test cohort were randomly recruited between March 13, 2000 and January 31, 2002 for immunohistochemistry (IHC) analysis. These resected samples were also subjected to western blot verification (n = 10). To verify immunohistochemical results of test cohort, another large-scale cohort as validation cohort, including 70 cases randomly recruited between February 18, 2002 and March 6, 2003, was analyzed via IHC. In addition, 43 HCC tissue samples and 43 liver cirrhosis tissue samples were randomly collected between February 18, 2002 and March 6, 2003, and used for further IHC expression analysis.

For the use of clinical materials for research purposes, prior patients' consents and approval were obtained from the Ethics Committee of Renji Hospital, Shanghai Jiao Tong University School of Medicine and EHBH of the Second Military Medical University. All experiments were performed in accordance with approved guidelines of Shanghai Jiao Tong University School of Medicine.

Immunohistochemistry and Scoring

Immunohistochemistry, signal evaluation, and integrated optical density (IOD) analysis were performed as described previously18. TDO antibody was purchased from Aviva Systems Biology (1:100) and KMO antibody was purchased from LifeSpan BioSciences (1:100). Photographs of three representative fields were captured under high-power magnification (×200); identical settings were used for each photograph. IOD was counted and measured using Image-Pro Plus v6.0 software, and mean IOD was calculated from three photographs per specimen.

Immunostaining scores were independently evaluated by two pathologists who were blinded to the clinical outcome. Semiquantitative scores were used to analyze immunostaining of each HCC case in tissue microarray. Intensity of staining was categorized into −, +, ++, or +++, denoting negative, weak, moderate, or strong staining, respectively. Extent of immunostaining was categorized into 0 (0–5%), 1 (6–25%), 2 (26–50%), or 3 (>51%) on the basis of the percentage of positive cells. Three random microscope fields per tissue were calculated. The sum of intensity and extent of staining was used as final score of expression level, and determined by the formula: final score = intensity score × percentage score. The final score of ≤3 was defined as low expression, and >3 as high expression.

Cell Culture and Transfection

Human normal liver cell lines L02 and SMMC7721 were obtained from Shanghai Institute of Cell Biology, Chinese Academy of Sciences. SK-Hep1 and PLC-PRF5 were purchased from the American Type Culture Collection. MHCC97H, MHCC97L, and HCCLM3 were provided by the Liver Cancer Institute of Zhongshan Hospital of Fudan University (Shanghai, China). Huh7 cells were purchased from Riken Cell Bank (Tsukuba, Japan). All the cell lines were cultured in Dulbecco’s modified Eagle’s medium (DMEM) (Gibco, Gaithersburg, MD, USA) containing 10% fetal bovine serum (FBS), 100 mg/ml penicillin, and 100 mg/ml streptomycin. All of the cells were incubated in a humidified atmosphere of 5% CO2 and 95% air at 37 °C. SK-Hep1 and MHCC-97H cells were transfected with KMO siRNA using lipofectamine 2000 (Invitrogen, Carlsbad, CA) according to the manufacturer’s instructions. SMMC7721 and Huh7 were transfected with the vector constitutively expressing KMO(pCMV6-XL5/KMO), or the control empty vector (pCMV6-XL5/Vector) according to the manufacturer’s instructions. The siRNA duplexes targeted KMO (siRNA#1: forward 5’-CCAAGGUAUUCCCAUGAGATT-3’, reverse 5’-UCUCAUGGGAAUACCUU- GGTT-3’; siRNA#2: forward 5’-CAGCCCAUGAUAUCUGUAATT-3’, reverse 5’-UUACAGAUAUCAUGGGCUGTT-3’) and scramble siRNA duplex (forward: 5’-UUCUCCGAACGUGUCACGUTT-3’; reverse: 5’-ACGUGACACGUUCGGA- GAATT-3’) were chemically synthesized by Biomics Biotechnologies Co. Ltd (Shanghai, China). The pCMV6-XL5/KMO and pCMV6-XL5/Vector were purchased from Origene (Rockville, MD).

RNA isolation and Real Time PCR

Total RNA was extracted using TRIzol reagent (Invitrogen) and reversely transcribed using PrimeScript™ RT Reagent Kit (TaKaRa Biotechnology). Real time polymerase chain reaction (Real Time PCR) was subsequently performed following the manual (TaKaRa Biotechnology). Expression levels were normalized against β-actin, and relative expression levels were displayed using 2-ΔΔCt method. Primer sequences used are as follows: KMO: Forward:TGCTGAGAAATACCCCAATGTG; Reverse: CTGACAGTTGAATAG

GCTCCATC; β-actin: Forward: TTGTTACAGGAAGTCCCTTGCC; Reverse: ATGCTATCACCTCCCCTGTGTG.

Western Blot Analysis

Briefly, tissue and cell samples were homogenated in a RIPA buffer (Qiagen, China). After centrifugation at 12,000 g, 4 °C for 30 min, 50 μg of protein samples were fractionated by sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) and transferred to nitrocellulose membranes. After blocking non-specific binding sites for 60 min with 5 % non-fat milk, the membranes were incubated with rabbit monoclonal antibody against KMO (1:1,800; LifeSpan BioSciences, Inc.), or β-actin (1:1,000;Santa Cruz) at 4 °C overnight, respectively, and subsequently, probed with HRP-conjugated anti-rabbit secondary antibody (1:5,000; Santa Cruz) for 45 min at room temperature. Chemiluminescence detection was performed using SuperSignal West Femto Maximum Sensitivity Substrate Kit 19 (Pierce). Membranes were exposed and recorded with Molecular Imager ChemiDoc XRS+System (Bio-Rad, CA, USA).

Cell Proliferation Assay

Cell proliferation was measured using the Cell Counting Kit-8 reagent (CCK-8, Dojindo, Japan). Cells were seeded into a 96-well plate at 2 ×103 cells per well with 100 μl complete medium and cultured at 37 °C. 10 μl CCK-8 solution was added to each well after 0, 24, 48 and 72 hours, respectively.

Migration Assay

Cell migration assays were performed using Transwell filter champers (BD Biosciences). 5 × 104 cells in 200 μl serum-free DMEM were seeded in the upper chamber of a transwell and 800 μl medium supplemented with 15% FBS was added to the lower chamber. After indicated time (12 hours for SK-Hep1, 24 hours for MHCC-97H, 20 hours for SMMC7721 and 20 hours for Huh7) of incubation at 37 °C, migrated cells were fixed and stained with a dye solution containing 0.1% crystal violet and 20% methanol. Cells adhering to the lower side of the inserts were counted and imaged through an IX71 inverted microscope (Olympus). Five random microscopic fields were counted per well for each group, and the experiments were repeated at least three times independently.

Invasion Assay

For in vitro invasion assay, transwell filter champers (BD Biosciences) and transwells coated with Matrigel (BD Biosciences) were utilized according to manufacturer’s instructions. 5 × 104 cells in 200 μl serum-free DMEM were seeded in the upper chamber of a transwell and 800 μl medium supplemented with 15% FBS was added to the lower chamber. After indicated time (20 hours for SK-Hep1, 40 hours for MHCC-97H, 24 hours for SMMC7721 and 30 hours for Huh7) of incubation at 37 °C, invaded cells were fixed and stained with a dye solution containing 0.1% crystal violet and 20% methanol. Cells adhering to the lower side of the inserts were counted and imaged through an IX71 inverted microscope (Olympus). Five random microscopic fields were counted per well for each group, and the experiments were repeated at least three times independently.

Statistic Analysis

Differences among variables were assessed by χ2 analysis or two-tailed Student t test. Kaplan-Meier analysis was used to assess survival. Log-rank tests were used to compare survival of patients between subgroups. Multivariate analyses were performed by multivariate Cox proportional hazard regression model. The experiments were performed in triplicates and data were presented as mean ± SEM. Differences were considered to be statistically significant for p < 0.05.

Results

Up-regulation of KMO in HCC tissues

KMO expression was first analyzed in 10 matched pairs of HCC and adjacent non-tumorous liver tissue by Western blotting. As shown in Fig. 1A, in most cases, KMO expression in HCC tissue was obviously higher than in adjacent non-tumorous liver tissue of the same HCC patient. We next performed IHC analysis for KMO using a tissue microarray as a test cohort, which contained 50 paired HCC tissue samples. Immunohistochemical results showed the staining density of KMO in HCC group was obviously stronger than that in adjacent non-tumorous liver tissue group (Fig. 1B,C, p < 0.05). We further analyzed KMO expression in another independent validation cohort of 70 HCC patients by IHC. Similarly, KMO expression was significantly increased in HCC group compared with adjacent non-tumorous liver tissue group (Fig. 1D,E, p < 0.05).

Figure 1. Up-regulation of KMO in HCC tissues.

Figure 1

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(A) Western blotting analysis for KMO in 10 paired samples of HCC tissues (T) and matched adjacent non-tumorous liver tissues (N). Left panel Representative Western blots for KMO and β-actin were shown. Right panel Band intensities of KMO were normalized to β-actin and showed as T/N Fold Change. Uncropped full-length blots for A are shown in the Supplementary Fig. 1. (B) IHC staining of KMO in 50 pairs of HCC tissues (T) and matched adjacent non-tumorous liver tissues (N) (Test cohort). (C) Integrated optical density (IOD) for KMO was obtained from the test cohort. (D) IHC staining of KMO in 70 pairs of HCC tissues (T) and matched adjacent non--tumorous liver tissues (N) (Validation cohort). (E) IOD for KMO was obtained from the validation cohort.

We also performed IHC analysis for KMO using a tissue microarray, which contained 43 tumor tissues from HCC patients and 43 liver tissues from liver cirrhosis patients. Our data showed that KMO expression exhibited a progressive increase from liver cirrhosis to HCC (Fig. 2A,B, p < 0.05).

Figure 2. Comparison of KMO levels in HCC patients and LC patients.

Figure 2

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(A) IHC staining of KMO in 43 HCC patients and 43 LC patients. (B) IOD for KMO was obtained from (A).

Association of KMO expression with clinicopathologic features in HCC patients

Next, we investigated relationship between KMO expression and clinicopathological variables of HCC patients. IHC was performed to assess KMO expression in a retrospective cohort with 205 HCC patients, including 59 cases of stage I (28.8%), 120 cases of stage II (58.5%), and 26 cases of stage III (12.7%), based on the TNM staging. KMO expression in the 205 samples was determined as high expression in 70 cases (70/205, 34.1%) and low expression in 135 cases (135/205, 65.9%). Spearman analysis revealed significant correlation between KMO and tumor differentiation (p = 0.004). However, there was no significant association between expression of KMO and other clinicopathological parameters such as age, sex, HBsAg status, tumor size, Child-Pugh, and vascular invasion (Table 1).

Table 1. Correlation between KMO expression and clinicopathologic parameters in HCC.

Variable (missing cases)   KMO protein    
  All cases Low expression High expression pvalue
Age       0.886
 ≤50 104 68 36  
 >50 101 67 34  
Sex       0.515
 Male 174 113 61  
 Female 31 22 9  
HBsAg       0.602
 Negative 54 34 20  
 Positive 151 101 50  
Serum AFP       0.316
 ≤20 ng/ml 74 52 22  
 >20 ng/ml 131 83 48  
Liver cirrhosis       0.932
 No 20 13 7  
 Yes 185 122 63  
TNM       0.299
 I 59 42 17  
 II 120 79 41  
 III–IV 26 14 12  
Child-Pugh class       0.777
 A 195 128 67  
 B 10 7 3  
Tumor size       0.268
 ≤3 cm 25 14 11  
 >3 cm 180 121 59  
Tumor number       0.118
 Single 162 111 51  
 Multiple 43 24 19  
Tumor differentiation(3)       0.004*
 I-II 37 32 5  
 III-IV 165 102 63  
Vascular invasion       0.155
 No 69 50 19  
 Yes 136 85 51  
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Chi-square test for comparison between groups. *p < 0.05. HBsAg, hepatitis B surface antigen; AFP, alpha-fetoprotein; TNM, tumor-node-metastasis

Correlation of KMO expression with prognosis of HCC patients

To determine the value of KMO for the prognosis of postsurgical HCC patients, Kaplan-Meier overall survival (OS) and time to recurrence (TTR) analyses were conducted. At the time of last follow-up, among the 205 HCC patients in the cohort, 118 had tumor recurrence and 120 had died. The mean OS was 48.7 months for patients with low KMO expression and 24.0 months for patients with high KMO expression. The mean TTR was 32.3 months for patients with low KMO expression and 16.2 months for patients with high KMO expression. These results indicated that patients with high KMO expression had much shorter OS times (Fig. 3A, p = 0.0005) and a higher tendency of disease recurrence (Fig. 3B, p = 0.0034). Moreover, we also performed IHC analysis for tryptophan 2,3-dioxygenase (TDO), which is the main KP enzyme in liver cells, using a tissue microarray with 182 HCC patients. Kaplan-Meier OS and TTR analyses were conducted and results showed that TDO had no prognostic value for postsurgical HCC patients (Supplementary Fig. 2).

Figure 3. Correlation of KMO expression with OS and TTR in HCC patients.

Figure 3

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(A) Representative photomicrographs showed negative (−), weak (+), moderate (++), or strong (+++) immunostaining of KMO in HCC specimens (magnification, × 50, × 200). (B, C) Kaplan-Meier curves of OS (B) and TTR (C) in 205 HCC patients.

Additionally, prognostic value of KMO was further confirmed by stratified OS and TTR analyses. Results showed that high expression of KMO was closely connected with OS and TTR after surgical resection in subgroups including TNM stage (TNM stage I , Fig. 4A,B; TNM stage II-III, Fig. 4C,D), tumor number (tumor number = 1, Fig. 4E,F), tumor size (tumor size >3 cm, Fig. 4G,H), and AFP concentration (AFP ≤20 ng/ml, Fig. 4I,J).

Figure 4. Correlation of KMO expression with OS and TTR in HCC subgroups.

Figure 4

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Analyses of OS and TTR by TNM stage (A–D), tumor number = 1 (E, F), Tumor Size >3 cm (G, H), and AFP ≤ 20 ng/ml (I, J).

Univariate and multivariate analyses of prognostic variables in HCC patients

We next evaluated prognostic significance of KMO and other clinicopathologic parameters in HCC using univariate analysis. As shown in Table 2, KMO as well as TNM stage, tumor number, tumor differentiation, and microvascular invasion, was responsible for the OS and TTR of HCC patients.

Table 2. Univariate and multivariate analysis of different prognostic parameters in patients with HCC by Cox regression analysis.

Factors OS
 TTR
    Multivariate
   Multivariate
  Univariate p HR 95%Cl   Univariate p HR 95% Cl p
Age: ≤50 vs >50 0.520 NA NA NA 0.420 NA NA NA
Sex: Male vs Female 0.244 NA NA NA 0.192 NA NA NA
HBsAg: Negative vs Positive 0.028 NA NA NA 0.168 NA NA NA
Serum AFP (ng/ml): ≤20 vs >20 0.215 NA NA NA 0.754 NA NA NA
Liver Cirrhosis : No vs Yes 0.307 NA NA NA 0.442 NA NA NA
TNM: I vs II vs III–IV 0.000 NA NA NA 0.001 1.633 1.216–2.192 0.001
Child-Pugh: A vs B 0.616 NA NA NA 0.509 NA NA NA
Tumor Size: ≤3 cm vs >3 cm 0.159 NA NA NA 0.774 NA NA NA
Tumor Number: Single vs Multiple 0.003 1.827 1.200–2.780 0.005 0.010 NA NA NA
Tumor Differentiation: I-II vs III-IV 0.041 NA NA NA 0.755 NA NA NA
Microvascular Invasion: No vs Yes 0.000 2.182 1.439–3.308 0.000 0.035 NA NA NA
KMO: Negative vs Positive 0.001 1.700 1.161–2.489 0.006 0.003 1.763 1.193–2.606 0.004
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Multiple Cox regression analysis was further utilized to evaluate independent prognostic value of KMO. Results revealed that KMO was an independent prognostic marker for OS (HR: 1.700, 95% CI: 1.161–2.489, p = 0.006) and TTR (HR: 1.763, 95% CI: 1.193–2.606, p = 0.004) in HCC patients (Table 2).

Inhibition of cell proliferation, migration, and invasion by KMO knockdown

We also assessed protein level of KMO in a normal liver cell line L02 and seven HCC cell lines, including SMMC7721, Huh7, SK-Hep1, PLC-PRF5, MHCC-97L, MHCC-97H, and HCC-LM3. Results showed that KMO expression was much higher in HCC cell lines, compared with the normal liver cell line L02 (Fig. 5A). Then, KMO was knocked down in SK-Hep1 and MHCC-97H cells, which expressed high levels of KMO, by small interfering RNA (siRNA). The mRNA and protein levels of KMO were effectively down-regulated by two KMO siRNAs at 48 hours of posttransfection (Supplementary Fig. 4 and Fig. 5B). As indicated by results of CCK8 assays (Fig. 5C), the proliferation of SK-Hep1 cells was significantly inhibited after KMO siRNAs transfection on day 2 (p < 0.05) and day 3 (p < 0.01). Likewise, compared to scramble siRNA transfected cells, proliferation of MHCC-97H cells also significantly inhibited after KMO siRNAs transfection on day 3 (p < 0.05). Besides, effects of KMO on cell migration and invasion were also investigated using transwell migration assays and matrigel invasion assays, respectively. Our results showed that KMO knockdown significantly decreased the migration and invasion rates of both SK-Hep1 and MHCC-97H cells in vitro, respectively (Fig. 5D,E, all p < 0.05).

Figure 5. Inhibition of proliferation, migration, and invasion by KMO siRNAs in vitro.

Figure 5

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(A) Analysis of KMO expression in HCC cell lines by Western blotting. Upper panel Representative Western blots for KMO and β-actin were shown. Lower panel Band intensities of KMO were normalized to β-actin and showed as Relative Intensity to L02 cells. Uncropped full-length blots were showed in the Supplementary Fig. 3. (B) SK-Hep1 and MHCC-97H cells were transfected with no siRNA (Mock), siRNA control (Scramble siRNA) or siRNAs against KMO (KMO siRNA#1 and KMO siRNA#2), respectively. Knockdown efficiency of KMO was verified by Western blotting. Upper panel Representative Western blots for KMO and β-actin were shown. Lower panel Band intensities of KMO were normalized to β-actin and showed as Relative Intensity to Mock cells, respectively. Uncropped full-length blots were showed in the Supplementary Fig. 5. (C) Cell proliferation of SK-Hep1 and MHCC-97H cells transfected with KMO siRNA was observed by CCK8 assay. (D) Cell migration of SK-Hep1 and MHCC-97H cells transfected with KMO siRNA was measured by transwell migration assays. (E) Cell invasion of SK-Hep1 and MHCC-97H cells transfected with KMO siRNA was measured by matrigel invasion assays. Data are mean ± SD of 3 biological replicates (*p < 0.05, **p < 0.01, ***p < 0.001).

Enhancement of cell proliferation, migration, and invasion by KMO over-expression

To further confirm the effects of KMO on proliferation, migration, and invasion, SMMC7721 and Huh7 cells were transfected with a vector constitutively expressing KMO (pCMV6-XL5/KMO) and a empty control vector (pCMV6-XL5/Vector), respectively. The mRNA and protein levels of KMO were significantly increased in pCMV6-XL5/KMO cells compared with pCMV6-XL5/Vector (Supplementary Fig. 6 and Fig. 6A). As indicated by results of CCK8 assays (Fig. 6B), the proliferation of SMMC7721 cells was significantly increased after KMO over-expression on day 3 (p < 0.05). Likewise, compared to empty control vector transfected cells, proliferation of Huh7 cells significantly increased after KMO over-expression on day 2 (p < 0.05) and day 3 (p < 0.01). Furthermore, KMO over-expression also significantly increased the migration and invasion rates of both SMMC7721 and Huh7 cells in vitro, respectively (Fig. 6C,D, all p < 0.01).

Figure 6. Enhancement of proliferation, migration, and invasion by KMO over-expression in vitro.

Figure 6

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(A) SMMC7721 and Huh7 cells were transfected with a vector constitutively expressing KMO (pCMV6-XL5/KMO) and a empty control vector (pCMV6-XL5/Vector), respectively. KMO expression was detected by Western blotting. Upper panel Representative Western blots for KMO and β-actin were shown. Lower panel Band intensities of KMO were normalized to β-actin and showed as Relative Intensity to pCMV6-XL5/Vector cells. Uncropped full-length blots were showed in the Supplementary Fig. 7 (B) Cell proliferation of SMMC7721 and Huh7 cells transfected with pCMV6-XL5/Vector and pCMV6-XL5/KMO were observed by CCK8 assay. (C) Cell migration of SMMC7721 and Huh7 cells transfected with pCMV6-XL5/Vector and pCMV6-XL5/KMO was measured by transwell migration assays. (D) Cell invasion of SMMC7721 and Huh7 cells transfected with pCMV6-XL5/Vector and pCMV6-XL5/KMO was measured by matrigel invasion assays. Data are mean ±SD of 3 biological replicates (*p < 0.05, **p < 0.01, ***p < 0.001).

Discussion

Despite substantial advances in surgery and chemotherapy for HCC in the past time3,19,20. therapeutic failure and mortality are still very common. The current pathological TNM (pTNM) stage and histological grading systems are established and can indicate HCC prognosis to a certain extent. However, due to tumor heterogeneity and accumulation of genetic and epigenetic alterations, patients with the same pTNM stage and/or histological grade of HCC often demonstrate considerable variability in tumor recurrence and metastasis21. Thus, searching for valuable diagnostic and prognostic predictors that can effectively distinguish between patients with favorable or unfavorable prognoses in the same stage and/or grade are urgently needed. Although previous studies have suggested several molecular biomarkers of HCC22,23,24,25,26, the novel biomarkers that can identify tumor recurrence and aid risk assessment remain substantially limited.

In the present study, we provide the first evidence that increased expression of KMO is correlated with an unfavorable clinical outcome of HCC patients. IHC staining in two independent cohorts (test cohort: 50 paired; validation cohort: 70 paired) indicated that KMO was abnormally elevated in HCC specimen compared with adjacent non-tumorous liver tissue. In a cohort of 205 HCC patients, Kaplan-Meier OS and TTR analyses showed that high KMO expression was associated with short HCC recurrence and poor prognosis after surgical resection. Multiple Cox regression analysis further conformed that KMO was an independent prognostic marker for OS and TTR. In addition, our data also showed a progressive increase of KMO from liver cirrhosis to HCC. These findings implicate that up-regulation of KMO may be a common feature in HCC and it can serve as an independent prognostic marker to identify patients with poor clinical outcome.

Identification of novel and specific prognostic biomarker for patients with early stage HCC is remarkably important27. Although AFP is most commonly employed and currently available as serological markers of HCC for surveillance, diagnosis and patient outcome prediction28,29,30, HCC patients without AFP elevation (AFP < 20 ng/ml) are missed and subsequently progress to late stage HCC before becoming clinically symptomatic and detectable28,30. Moreover, the diagnostic and prognostic sensitivity of AFP was poor in the early stage of HCC, especially when used alone. Here, we evaluated the clinical usefulness of KMO as a prognostic factor in HCC patients with AFP < 20 ng/ml, which accounted for 36.1% of HCC patients in our study cohort. In addition, our results also showed that high expression of KMO in HCC patients at TNM I stage was closely associated with the risk of recurrence and shorter survival time (OS, p = 0.0042; TTR, p = 0.0500). Thus, our results have exhibited the potential value of KMO in predicting the risk of recurrence and patient survival in subgroups with normal AFP levels (AFP < 20 ng/ml) or in the early-stage HCC group, which would have been difficult using currently clinically available surrogate biomarkers.

Molecular mechanisms underlying recurrence or metastasis of HCC are very complicated. Genetically, chromosomal copy number alterations, such as the loss of alleles on 16q and the amplification of 1q, have been found to associate with HCC metastasis31,32. Recently, multiple genes associated with HCC progression and metastasis have also been identified, including PGE233, Keratin 1934, FoxQ135, ICAT36, and Gankyrin37. KMO locates in a pivotal position in KP, which is responsible for >95% of tryptophan degradation in mammals, ultimately leading to the formation of NAD38,39. NAD is a key regulator of several energy and signal transduction processes such as transcription, DNA repair, cell cycle progression, apoptosis and metabolism, which are relevant to tumor cell survival and proliferation. It functions as a coenzyme in metabolic pathways including glycolysis and the pentose phosphate pathway, thereby allowing the efficient production of NADPH, ribose-5-phosphate (Rib-5-P) and biosynthetic compounds used by the tumor for growth and angiogenesis40. Moreover, aberrant NAD metabolism is considered a hallmark of cancer: the high rates of aerobic glycolysis (Warburg effect) perturbs NAD metabolism, thereby leading to disrupt the cellular NADH/NAD+ redox homeostasis, and promote cancer progression41,42. Our data first exhibited that KMO expression was significantly upregulated in HCC tissues. As a pivotal enzyme in the kynurenine pathway, increased KMO expression might affect NAD concentration in HCC and then involved in HCC progression.

Previous studies showed that modulation of KMO activity was mainly involved in several neurodegenerative diseases, including Huntington's disease and Alzheimer's disease6,43. However, roles of KMO in tumor, including HCC, remain hitherto unknown. It has been previously reported that selective degradation of tryptophan created an immunosuppressive micromilieu of tumor both by depleting tryptophan and by accumulating immunosuppressive metabolites of the kynurenine pathway: On the one hand, tryptophan shortage inhibited T cells proliferation and causes a lack of accumulation of specific T cells at the tumor site44,45. On the other hand, the main tryptophan metabolites, such as Kynurenine, 3-hydroxykynurenine, and 3-hydroxyanthranilic acid, could suppress the T cell response and kill T cells, B cells and natural killer (NK) cells46,47. In this study, we found that KMO expression positively regulated proliferation, migration and invasion of HCC cells in vitro. Although underlying mechanism remains to be further investigated, our present study provides a clue for biological function of KMO in HCC.

To the best of our knowledge, this is the first study to report that high KMO expression is correlated with aggressive malignant phenotype of HCC. Our data indicate that KMO may serve as a novel prognostic marker for HCC and targeting KMO may provide a promising strategy for HCC treatment.

Additional Information

How to cite this article: Jin, H. et al. Prognostic significance of kynurenine 3-monooxygenase and effects on proliferation, migration, and invasion of human hepatocellular carcinoma. Sci. Rep. 5, 10466; doi: 10.1038/srep10466 (2015).

Supplementary Material

Supplementary Information
srep10466-s1.doc (900.5KB, doc)

Acknowledgments

National Natural Science Foundation of China (81371883 and 81201627), the Shanghai Natural Science Foundation of China (13ZR1440300), Shanghai Health Bureau Youth Fund (2009Y110), Shanghai Municipal Program of International Cooperation in Science and Technology (12410709800), Research Fund for the Doctoral Program of Higher Education of China (20120073110091), the Doctoral Innovation Fund of Shanghai Jiao Tong University School of Medicine (BXJ201319)

Footnotes

Author Contributions W.X.Q. and W.M.C. designed the study; H.J.J., H.Y.Y., Y.R.Z. and G.Z.J. collected the tissue samples; H.J.J., Y.R.Z., H.Y.Y., N.W. and H.Y.R. performed the cell culture, cell transfection and WB test; H.J.J., D.S.G. and X.S.H. carried out cell proliferation assay, migration assay and invasion assay. Y.R.Z., X.M.T and C.W. performed and evaluated the IHC analysis; H.J.J., C.W. and G.Z.J. collected clinical data and participated in the evaluation of the IHC data; H.J.J. drafted the manuscript; W.X.Q. and W.M.C. supervised the study. All authors read and approved the final manuscript.

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