Background
Gastric cancer (GC) is the fourth most common cancer and the second leading cause of cancer-related death worldwide [
1]. Recent improvements in diagnostic tools and methods have facilitated detection of early GC and thereby excellent long-term survival. However, patients with advanced disease at the time of diagnosis remain poor outcomes. Metastasis is a multistep process, involving local invasion, dissemination, and re-establishment into distant organs, and is the major determinant of the mortality [
2]. Therefore, a better understanding of metastasis may open the way to a host of innovative therapeutic strategies in GC.
The protein tyrosine phosphatases (PTPs) form a large family of enzymes that serve as key regulatory components in signal transduction pathways [
3]. The phosphatases of regenerating liver (PRL-1, -2, and -3), belonging to a small class of PTP superfamily, have a unique COOH-terminal prenylation motif, which critically affects their cellular localization and function [
4]. PRL-3 was firstly identified to be specifically over-expressed in liver metastases derived from colorectal cancer [
5], and subsequently its overexpression was documented in various tumor types, including GC [
6]. PRL-3 can promote cancer invasion, migration, growth, and angiogenesis, through either dephosphorylation that is catalyzed by catalytic domain or localization to plasma membrane directed by COOH-terminal prenylation motif [
7‐
9]. Thus, PRL-3 has deserved attention as a crucial molecule in the multiple steps of metastasis and therefore as a new therapeutic target. On the other hand, the mechanisms inducing PRL-3 expression are not fully clarified. Amplification of genomic regions containing oncogenes is the major mechanism of its consequent overexpression and the cancer development, and therefore has importance for targeted therapies [
10].
PRL-3 gene amplification partially accounts for the overexpression in colorectal cancer and esophageal cancer [
5,
11]. However, the relationship between genomic amplification and GC remains elusive in the both mechanistic and therapeutic points of view. In the present study, we examined the characteristics of
PRL-3 genomic amplification in GC, and further assessed the clinical potential of PRL-3-targeted therapy.
Methods
Cell lines and Tissue Samples
The GC cell line MKN7 was kindly provided from the Cell Resource Center for Biomedical Research Institute of Development, Aging and Cancer, Tohoku University (Sendai, Japan). Seven other GC cell lines (GCIY, AZ521, KatoIII, SH10, H111, MKN74, and NUGC4) were purchased from RIKEN BioResource Center (Ibaraki, Japan). These cell lines cover the two main types of GC [
12], intestinal type (MKN7, MKN74, AZ521, and H111 cells) and diffuse type (GCIY, KatoIII, SH10, and NUGC cells) [
13‐
15]. MKN7, NUGC4, and AZ521 cells were established from lymph node metastasis (LNM), and MKN74 cells were from liver metastasis. KATOIII and GCIY cells were established from metastatic pleural effusion and ascites, respectively. H111 and SH10 cells were established from the xenotransplantation. Normal skeletal muscle C2C12 cells were purchased from DS Pharma Biomedical Co., Ltd (Osaka, Japan). AZ521 and C2C12 cells were grown in DMEM medium (GIBCO, Carlsbad, CA) supplemented with 10% fetal bovine serum (FBS). The other cells were grown in RPMI1640 medium (GIBCO) supplemented with 10% FBS. 1-4-bromo-2-benzylidene rhodanine was purchased from Calbiochem Corp (San Diego, CA), which was identified as a PRL-3 inhibitor through high throughput screening using chemical library of Korea Chemical Bank, and inhibited PRL-3 phosphatase activity [
16]. Indeed, phosphorylation of KRT8, PRL-3-interacting protein, induced by catalytically inactive mutant of PRL-3, but not by wild type, was confirmed by PRL-3 inhibitor treatment in a dose-dependent manner [
17]. Moreover, anticancer efficacy of PRL-3 inhibitor treatment also showed to be similar to that of siRNA treatment in esophageal cancer or colorectal cancer [
11,
17].
Out of 173 formalin-fixed, paraffin-embedded, tissue samples series where we previously assessed PRL-3 expression status using immunohistochemical staining (IHC) in GC [
6], 77 matched pairs of primary tumor tissues and the corresponding normal mucosa tissues were randomly selected from patients with differential stages according to the 13
th edition of the Japanese Classification of Gastric Carcinoma (JCGC) [
18]; 40 pairs with positive PRL-3 expression (10 patients in Stage I, 10 in II, 10 in III, and 10 in IV) and 37 pairs with negative expression (10 patients in stage I, 10 in II, 9 in III, and 8 in IV). All patients underwent gastrectomy according to the gastric cancer treatment guidelines in Japan [
19], and histopathologic examinations were done according to the JCGC. The 6
th edition of the International Union Against Cancer (UICC)/TNM classification was also used [
20]. Table
1 depicts the detailed information on 77 patients. All tissue samples were collected at the Kitasato University Hospital, and informed consent was obtained from all patients. The present study was approved by the Ethics Committee of the Kitasato University.
Table 1
Correlation between PRL-3 gene amplification and clinicopathological variables in 77 patients with gastric cancer
PRL-3 expression | | | | | | 0.006 |
Negativity | 37 | 37 | (100) | 0 | (0) | |
Positivity | 40 | 32 | (80) | 8 | (20) | |
Age (years) | | | | | | 0.726 |
<60 | 34 | 30 | (88) | 4 | (12) | |
≥60 | 43 | 39 | (91) | 4 | (9) | |
Gender | | | | | | 0.710 |
Male | 51 | 45 | (88) | 6 | (12) | |
Female | 26 | 24 | (92) | 2 | (8) | |
Lymphatic permeation | | | | | | 0.343 |
Absence | 15 | 15 | (100) | 0 | (0) | |
Presence | 62 | 54 | (87) | 8 | (13) | |
Vascular permeation | | | | | | 0.263 |
Absence | 25 | 24 | (96) | 1 | (4) | |
Presence | 52 | 45 | (87) | 7 | (13) | |
Differentiation | | | | | | 0.134 |
Well and moderate | 31 | 30 | (97) | 1 | (3) | |
Poor | 46 | 39 | (85) | 7 | (15) | |
Depth of invasion | | | | | | 0.006* |
T1 (m and sm) | 15 | 15 | (100) | 0 | (0) | |
T2 (mp and ss) | 35 | 33 | (94) | 2 | (6) | |
T3 (se) | 19 | 16 | (84) | 3 | (16) | |
T4 (si) | 8 | 5 | (63) | 3 | (38) | |
Lymph node metastasis | | | | | | 0.022 |
Absence | 29 | 29 | (100) | 0 | (0) | |
Presence | 48 | 40 | (83) | 8 | (17) | |
JCGC lymph node status†
| | | | | | 0.004* |
N0 | 29 | 29 | (100) | 0 | (0) | |
N1 | 21 | 20 | (95) | 1 | (5) | |
N2 | 20 | 14 | (70) | 6 | (30) | |
N3 and distant lymph nodes | 7 | 6 | (86) | 1 | (14) | |
UICC lymph node status‡
| | | | | | 0.002* |
N0 | 29 | 29 | (100) | 0 | (0) | |
N1 | 18 | 17 | (94) | 1 | (6) | |
N2 | 16 | 13 | (81) | 3 | (19) | |
N3 and distant lymph nodes | 14 | 10 | (71) | 4 | (29) | |
JCGC stage | | | | | | 0.005* |
I (IA and IB) | 20 | 20 | (100) | 0 | (0) | |
II | 20 | 20 | (100) | 0 | (0) | |
III (IIIA and IIIB) | 19 | 15 | (79) | 4 | (21) | |
IV | 18 | 14 | (78) | 4 | (22) | |
UICC stage | | | | | | 0.003* |
I (IA and IB) | 21 | 21 | (100) | 0 | (0) | |
II | 20 | 20 | (100) | 0 | (0) | |
III (IIIA and IIIB) | 16 | 13 | (81) | 3 | (19) | |
IV | 20 | 15 | (75) | 5 | (25) | |
Fluorescence in situ hybridization analysis
Fluorescence in situ hybridization (FISH) analysis was performed, as described previously [
11].
PRL-3 is located on chromosome 8q24.3 (GenBank accession number NT 000008.9), and the chromosome 8 centromeric probe was used to estimate the copy number. Because
PRL-3 FISH scoring algorithms had not been standardized, the assessment was based on the criteria of
HER2 [
21]. For each sample, at least 60 cancer cells were scored. Positive
PRL-3 genomic amplification was defined as a ratio of
PRL-3 to chromosome 8 centromere more than 2.2, and negative was the ratio of less than 1.8. If the ratio of
PRL-3 to chromosome 8 centromere was 1.8 to 2.2, additional cells were counted, and the ratio of more than 2.0 was finally considered as positive [
21]. Polysomy was defined as the mean chromosome 8 centromeric signals more than 3.0 per nucleus [
22].
Quantitative-genomic PCR
Tissue sections from tumor and the corresponding normal mucosa, obtained at least 5 cm from the tumor edge, were sharply dissected on hematoxylin and eosin-stained slides, and genomic DNA was subsequently extracted using of a QIAamp DNA FFPE Kit (QIAGEN Sciences, Hilden). Quantitative-genomic polymerase chain reaction (Q-PCR) was performed to quantify
PRL-3 gene copy numbers using iQ™ Supermix (Bio-Rad Laboratories, Hercules, CA) in triplicate on the iCycler iQ™ Real-Time PCR Detection system (Bio-Rad). To normalize
PRL-3 gene copy number per cell, ADAM metallopeptidase domain 2 (
ADAM2, NT 923907.1), located on chromosome 8p11.2, was used as an endogenous reference because that gene amplification is defined as a copy number increase of a restricted region of a chromosome arm [
10]. ∆Ct values were calculated as Ct (
PRL-3)-Ct (
ADAM2) for each sample. Relative copy number was determined as 2
-
∆∆
Ct, where ∆∆C
t = ∆C
t (tumor)-∆C
t (corresponding normal) [
23]. The increases of more than 2-fold relative to the corresponding normal were considered as genomic amplification. Additional file 1 depicts detailed PCR condition and sequences of primer and probe used in the present study.
Western blotting
Whole cell lysates were extracted in RIPA buffer (Pierce, Rockford, IL) supplemented with 10 μL/mL Halt™ Protease Inhibitor Cocktail Kit (Pierce) and Halt™ Phosphatase Inhibitor Cocktail Kit (Pierce), and the protein were separated on NuPAGE
® 4-12% Bis-Tris Gel (Invitrogen) according to the manufacturer's protocol. Both detection and quantification of the specific proteins were performed using ATTO Light Capture (ATTO Corporation, Tokyo, Japan). Two colorectal cancer cell lines DLD-1 and SW480 cells (RIKEN BioResource) were used as the low and high expression controls, respectively, as described previously [
11].
PRL-3 mouse monoclonal antibody (R&D Systems, Minneapolis, MN) and β-actin mouse monoclonal antibody (Sigma, St. Louis, MO) were used as described previously [
11].
PRL-3 small interfering RNA transfection
Cells were transfected with 1 μmol/L Accell SMARTpool, siRNA-PRL-3 (Thermo Fisher Scientific, Lafayette, CO) mixed with Accell siRNA Delivery Media (Thermo Fisher Scientific) according to the Thermo Scientific Dharmacon
® Accell™ siRNA Delivery Protocol [
24]. The Accell Non-targeting Pool (siRNA-ctr) and Accell siRNA Delivery Media alone were used as a control for non-sequence-specific effects and as a mock-treatment, respectively.
Anchorage-independent colony formation assay
Anchorage-independent cell growth was analyzed by plating 0.36% top agarose (Bacto™ Agar, Becton, Dickinson and Company, Franklin Lakes, NJ) containing 1 × 10
5 cells on a surface of 0.72% bottom agarose in 6-well plates [
11]. Cells were fed weekly by overlying fresh soft-agar solution, and colonies were photographed after 2 weeks of incubation. The 50% effective concentration (EC
50) value of PRL-3 inhibitor treatment was calculated based on the measurement of colony count.
Proliferation assay and invasion assay
The proliferation assay was performed using Premix WST-1 Cell Proliferation Assay System (Takara Bio, Tokyo). Cells (2 × 103) were seeded in 96-well, and the proliferative activity was measured by absorbance at 450 nm on designated sampling days. The sensitivity to PRL-3 inhibitor on antiproliferation was determined using the 50% inhibitory concentration (IC50) value after treatment for 72 hours.
The invasion assay was performed in the 24-well BD BioCoat™ Matrigel™ Invasion Chamber (BD Biosciences Discovery Labware, Bedford, MA). Cells that had invaded through the membrane were counted in four separated fields per well. Both experiments were done in triplicate.
Apoptosis Assays
Apoptosis assays were performed using Guava PCA System (Guava Technologies, Inc., Hayward, CA). Cells (2 × 105) were treated with the PRL-3 inhibitor at the indicated concentration in medium supplemental with 1.0% FBS for 72 hours, then stained with Annexin V and 7-AAD (Guava Nexin Reagent). The experiment was done in triplicate and analyzed using CytoSoft 2.1.5 software (Guava Technologies).
Statistical Analysis
Fisher's exact test, or the Mann-Whitney U-test was used to statistically analyze the relationship between PRL-3 gene amplification and clinicopathological variables. One-way analysis of variance (ANOVA) with post-hoc test was used to compare between three groups for siRNA treatment (siRNA-PRL-3, siRNA-ctr, and mock). Student t test was used to evaluate therapeutic effect for the individual concentrations of PRL-3 inhibitor, compared with 0 μmol/L of PRL-3 inhibitor. The Kaplan-Meier method was used to estimate cumulative survival rates, and differences in survival rates were assessed with the use of the log-rank test. All deaths of patients were cancer-related, and disease specific survival (DSS) was measured from the date of surgery to the date of death or the last follow-up. P < 0.05 was considered to indicate statistical significance. All statistical analyses were conducted with JMP 7.0 software (SAS Institute, Cary, NC).
Discussion
As LNM is considered as an important prognostic factor for GC [
29], research of the causative molecules reflecting LNM is a promising avenue to improve the outcomes. The close link of LNM with PRL-3 expression, therefore, has potential as a new therapeutic target [
6,
25]. However, the criteria for PRL-3-targeted therapy have not been established, and it is critical to clarify the characteristics of
PRL-3 genomic amplification in the both mechanistic and therapeutic points of view, because of the major mechanism of its consequent expression and the cancer development [
10]. In the present study, we offer the vital clues for the development of this therapeutic strategy against GC.
The relationship between PRL-3 expression and its genomic amplification have never been examined so far.
PRL-3 genomic amplification was concordant with its expression status in cell lines, and was found in 20% (8/40) among human primary tumors with expression, which were all stage III or IV disease (40%, 8/20), but in none (0/37) among those without expression. Additionally,
PRL-3 genomic amplification was associated with LNM status, leading to advanced stage and thereby poor outcomes in patients with LNM (
P = 0.021). Thus,
PRL-3 genomic amplification may be the more relevant alteration for LNM, and be one of the predominant mechanisms inducing its expression in the more advanced stage. However, most tumors expressing PRL-3 were not amplified, especially in the earler stage. In mouse embryonic fibroblast cells with wild type but not p53
-/-, PRL-3 is induced in a p53-dependent manner [
30]. The p53 mutation or loss of function, however, has been documented in all the GC cell lines used in the present study, except for NUGC4 cells (The TP53 Web Site,
http://p53.free.fr/), indicating that there is other mechanism independently of p53 pathway. PRL-3 expression was reported to be regulated at transcriptional level by mitogenic cytokines, such as IL-6, IL-21, HGF or IGF-1 in myeloma cell lines [
24], or as TGF-β in colon cancer cell lines [
31]. Recently, PolyC-RNA-binding protein 1 (PCBP1) has been identified as a translational regulator of PRL-3 [
32]. The alternative mechanisms at transcriptional or translational level may be involved to regulate PRL-3 expression.
We also confirmed that siRNA-mediated PRL-3 knockdown significantly repressed cell proliferation and invasion in line with previous reports for other GC cell lines [
25,
27], and furthermore for the first time revealed the reduced effect of colony formation under anchorage-independent conditions, supporting that PRL-3 may be attractive therapeutic target against GC. The success of molecular-targeted therapy depends on the identification of a landmark to select patients with more benefit from the therapy, such as activating mutation or gene amplification of EGFR in non-small cell lung cancer [
33], and overexpression or gene amplification of HER2 in breast cancer [
34]. Thus, genetic alteration or expression status is possible to be a landmark for molecular-targeted therapy, and it is indispensable to evaluate the anticancer activity of PRL-3 inhibitor treatment against cancer cells with different genetic and expression status. Although neither
PRL-3 genomic amplification nor expression level was responsible for the sensitivity to PRL-3 inhibitor treatment, the inhibitor exhibited dose-dependent efficacy on all the tested cell lines with PRL-3 expression, and remarkably induced apoptosis in line with a previous report [
35]. PRL-3 is not expressed in human adult stomach, and its expression is cancer-specific event [
6,
7]. Collectively, the presence of PRL-3 expression, but not expression level, may be sufficient to promote metastatic properties through activation of downstream signaling pathways, and the effective inhibition seems to have important implication for the success of this treatment. Combined with our previous findings demonstrating the high frequency of PRL-3 expression (55%, 95/173) [
6], PRL-3-targeted therapy may be applicable for most patients with GC. The different sensitivity against PRL-3 targeting as shown in the present study may imply the additional alterations attenuating the dependence of PRL-3 signaling networks on cancer cells. Therefore, identification of molecules leading to the different sensitivity would shed light on the development of more sophisticated strategy.
Normal tissues with PRL-3 expression may be susceptible to adverse effects from the targeted therapy, especially in normal skeletal muscle and heart [
28]. Interestingly, PRL-3 inhibitor treatment with the concentration of 10 μmol/L significantly repressed proliferation through apoptosis induction on all the tested GC cell lines, whereas did not on normal skeletal muscle C2C12 cells, implying that this concentration may act as an optimal dose of anticancer activity without severe effects against muscle cells, and normal cells may have a better apoptotic protective mechanism, even though PRL-3 is constitutively expressed [
35]. As C2C12 cells might not be the best control because of relatively weak expression, further research will be necessary to validate our findings.
Competing interests
The authors declare that they have no competing interests.
Authors' contributions
AO conceived of the study, performed the study, drafted the manuscript and participated in coordination. KY participated in coordination and assisted in editing of manuscript. SK, SS, NK, MW, HK, and KN helped in the collection and analysis of clinical data. MW participated in coordination. All authors read and approved the final manuscript.