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The expression of small, non-coding RNA, or microRNAs (miR), is frequently deregulated in human cancer, but how these pathways affect disease progression is still largely elusive. Here, we report on a microRNA, miR-296, which is progressively lost during tumor progression, and correlates with metastatic disease in colorectal, breast, lung, gastric, parathyroid, liver and bile ducts cancers. Functionally, miR-296 controls a global cell motility gene signature in epithelial cells by transcriptionally repressing the cell polarity-cell plasticity module, Scrib. In turn, loss of miR-296 causes aberrantly increased and mislocalized Scrib in human tumors, resulting in exaggerated random cell migration, and tumor cell invasiveness. Re-expression of miR-296 in MDA-MB231 cells inhibits tumor growth, in vivo. Finally, miR-296 or Scrib levels predict tumor relapse in hepatocellular carcinoma patients.
These data identify miR-296 as a global repressor of tumorigenicity, and uncover a previously unexplored exploitation of Scrib in tumor progression in humans.
A network of small, non-coding RNA or microRNAs (miR) has attracted attention as regulators of gene expression (Bartel, 2004), influencing human diseases (Garzon et al., 2009). In cancer, the systematic cataloging of deregulated miR expression in transformed cells compared to normal tissues (Lu et al., 2005), has helped uncovering novel transcriptional networks relevant to cell invasion (Valastyan et al., 2009) and metastasis (Zhang et al., 2010), as main drivers of unfavorable disease outcome in humans (Calin and Croce, 2006).
In this context, perturbation of a normal apical-basal polarity in epithelial cells (Etienne-Manneville, 2008) is thought of as one of the earliest phenotypical changes in cellular transformation (Zhan et al., 2008; Ouyang et al., 2010), heralding invasive cancer (Hanahan and Weinberg, 2000). The transcriptional programs underlying this process are not completely understood, but so-called cell polarity-cell plasticity modules, for instance the mammalian homologs of Drosophila melanogaster Scribble (Scrib), atypical protein kinase C (aPKC) or Crumbs (Crb) play a key role in apical-basal polarity of epithelia, cell orientation (Etienne-Manneville, 2008), and directional cell movements (Petrie et al., 2009). In this context, loss of polarity proteins in Drosophila (Bilder et al., 2000), or mammalian cells (Etienne-Manneville, 2008), deregulates cell proliferation (Dow et al., 2008; Wu et al., 2010), survival (Zhan et al., 2008), epithelial-mesenchymal transition (Bahri et al., 2010), and random cell migration (Osmani et al., 2006), suggesting that these molecules may function in an evolutionary-conserved pathway of tumor suppression, in vivo (Humbert et al., 2008; Wu et al., 2010).
In this study, we aimed at identifying novel miR regulators of tumor progression conserved in animal models and in epithelial human cancers irrespective of the cancer origin. We found that miR-296, a miR previously associated with angiogenic endothelial cells (Wurdinger et al., 2008), or to prostate cancer (Wei et al., 2010), functions as a global repressor of tumorigenicity, and that this pathway, differently from previous models (Humbert et al., 2008; Wu et al., 2010), involves deregulation and subcellular mislocalization of Scrib in metastatic human cancer (Etienne-Manneville, 2008).
We began this study by profiling the expression of 132 orthologous miRs in microdissected pancreatic islets isolated from Rat Insulin Promoter-T Antigen (RIP-TAg) transgenic mice (Hanahan, 1988), an established model of tumor progression, suitable for miR analysis (Olson et al., 2009). Islets from RIP-TAg mice exhibited extensive changes in miR expression during oncogenic transformation (4–6 weeks) and evolution to invasive pancreatic islet cell carcinoma (10 weeks) (Supplementary Figure 1a). In this analysis, miR-296 was consistently downregulated throughout all stages of islet tumorigenesis, in vivo (Figure 1a). Conversely, miR-296 was expressed at comparable levels in non-transgenic (NT) islets at the same time intervals (Figure 1a). As control, oncogenic miRs, including miR-21 (Seike et al., 2009) (Supplementary Figure 1b), or miR-19a (Supplementary Figure 1c) (Olson et al., 2009), were up-regulated in transgenic islets, but not aged-matched controls. In addition, unrelated miRs, for instance miR-452 (Supplementary Figure 1d), or miR-216 (Supplementary Figure 1e) were indistinguishably expressed in non-transgenic or RIP-TAg pancreatic tissues.
When analyzed in human samples, miR-296 levels were profoundly repressed in various cultured tumor cell lines representative of breast, lung, colorectal or liver adenocarcinoma, compared to normal mammary epithelial cells (HMEC) (Supplementary Figure 2a). Similarly, miR-296 expression was progressively lost in 86% of patient samples representative of the colorectal adenoma-to-carcinoma transition (13 out of 16 patients, P=0.0007, Table 1), compared to matched normal mucosa (Figure 1b). A comparable pattern was observed in disparate, genetically heterogeneous tumor types (Table 1), where miR-296 expression was frequently lost in primary (13 out of 20 patients, P<0.05), as well as metastatic lesions (15 out of 20 patients, P=0.009) (Table 1 and Supplementary Figure 2b). When correlated to disease outcome, loss of miR-296 levels in patients with hepatocellular carcinoma (HCC) (Augello et al., 2009), compared to matched normal liver (Figure 1c), was associated with considerably shortened disease-free survival (HR=2.4, Figure 1d).
Manipulation of miR-296 levels by transfection of antagomir (a-miR-296, Supplementary Figure 3a), or, conversely, pre-miR-296 (p-miR-296, Supplementary Figure 3b) had no effect cell cycle transitions in various tumor types, by DNA content analysis and flow cytometry (Supplementary Figure 3c). Conversely, antagomir depletion of miR-296 potently stimulated the migration of HMEC or breast adenocarcinoma MDA-MB231 and MCF-7 cells in a wound healing assay, in vitro (Figure 2a and Supplementary Figure 4a). This was also associated with enhanced invasion of HMEC (Figure 2b) or MDA-MB231 cells (Supplementary Figure 4b,c) across Matrigel-coated inserts, using serum (Supplementary Figure 4b), or co-culture with primary carcinoma-isolated fibroblasts (Supplementary Figure 4c) as chemotrattactants. Cells depleted of miR-296 also exhibited increased colony formation in soft agar (Figure 2c, Supplementary Figure 4d), another marker of tumorigenicity. Reciprocally, forced expression of miR-296 by transfection of p-miR-296 repressed breast epithelial cell migration (Figure 2a), invasion (Figure 2b, Supplementary Figure 4b,c), colony formation in soft agar (Supplementary Figure 4d), and promoted anoikis in breast cancer cells (Supplementary Figure 4e,f). In these experiments, perturbation of miR-296 levels induced defects in cellular orientation, as judged by the position of the Golgi apparatus relative to the nucleus (Figure 3a,b), and affected the formation of polarized actin protrusions at the leading edge of directional cell migration (Figure 3c,d). Finally, we tested whether miR-296 re-expression in MDA-MB231 cells (Figure 4a) also inhibits tumor growth. We injected control miRNA and mir-296 transfected cells into the fourth mammary fat pads of immunocompromised mice and monitored tumor growth for three weeks (Figure 4b). Mice injected with miR-296 re-expressing cells resulted in reduced tumor growth compared with controls (Figure 4c).
Consistent with the role of miRs in transcriptional control, changes in miR-296 levels had profound effects on the gene expression profile of tumor cells, as revealed by unsupervised clustering of candidate genes putatively modulated by miR-296 (Figure 5a). Out of 107 predicted candidate genes (Supplementary Table 1), potentially associated with miR-296 pathways (Supplementary Table 2), a 32-gene signature was validated by quantitative PCR in cells with acute changes in miR-296 expression (Figure 5a), comprising general regulators of tumor cell motility, migration, invasion, and metastasis (Figure 5b, Supplementary Table 1).
One of the target genes in the miR-296 gene signature was identified as the cell polarity-cell plasticity module, Scrib (Dow et al., 2007), an important regulator of apical-basal polarity and directional cell movement (Osmani et al., 2006). Accordingly, transfection of miR-296 suppressed Scrib protein expression in normal or transformed epithelial cells (Figure 6a and Supplementary Figure 5a), and significantly inhibited Scrib 3′ UTR activity in luciferase reporter assays (Figure 6b). In addition, mutagenesis of putative miR-296 binding site in Scrib identified by sequence analysis (Supplementary igure 5b) restored 3′ UTR activity to the levels of control transfectants (Figure 6b), validating Scrib as a target gene directly repressed by miR-296. Other putative or predicted target proteins as BMP8A (Supplementary Table 1) or HMGA1 (Wei et al., 2010), were not significantly modulated by miR-296 in our system (Supplementary Figure 5c).
Functionally, depletion of Scrib by small interfering RNA (siRNA) inhibited migration of MDA-MB231 cells in a wound healing assay, in a response unaffected by the caspase inhibitor Z-VAD (Figure 6c). In addition, Scrib knockdown blocked tumor cell invasion across Matrigel-coated inserts (Figure 6d), induced anoikis (Supplementary Figure 5d,e), prevented a correct cellular orientation towards the leading edge of migration, and reduced the number of polarized actin protrusion at the leading edge of the cell (Figure 6e,f). In contrast, a control, non-targeting siRNA had no effect on cell migration (Figure 6c), invasion (Figure 6d), or requirements of cellular motility (Figure 6e,f).
Mirroring the loss of miR-296 expression in human cancer, Scrib levels were conversely upregulated in primary lesions and distant metastases of colon, lung, breast, and stomach cancer (n=18), as well as HCC (n=62) (Augello et al., 2009), compared with matched normal mucosa (Figure 7a, Supplementary Figure 6a). k-Ras mutations on codon 12, RasV12, or 13, RasV13, identified in six patients with colon cancer (40%), did not correlate with expression of miR-296 (P=0.8, Fisher exact test, Table 1), or its target, Scrib. Scrib protein levels were also increased in hyperplastic, angiogenic and invasive β-islets from RIP-TAg mice compared to control (4-weeks old RIP-Tag) or non-transgenic littermates (Supplementary Figure 6b). In immunohistochemical studies on tumor specimens, the subcellular localization of Scrib was also deregulated, changing from a predominantly membranous localization at cell-cell junctions, and characteristic of the normal mucosa, to a diffuse cytoplasmic staining in primary and metastatic tumor cells (Figure 7a and Supplementary Figure 6a).
In terms of disease outcome, high levels of Scrib mRNA or protein expression in our series of HCC patients compared to normal liver (Figure 7b,c) significantly correlated with shortened overall survival (Figure 7d,e), thus mirroring the results with miR-296 expression in the same patient cohort (Figure 1d).
In this study, we have shown that miR-296, a miR initially associated with angiogenic responses (Wurdinger et al., 2008), is frequently lost during tumor progression in a mouse model of disease, and in primary human specimens, correlating with worse. Functionally, loss of miR-296 deregulates a global cell polarity-cell plasticity module, resulting in aberrant over-expression and mislocalization of Scrib in the transformed cell population (Etienne-Manneville, 2008), and enhanced tumor cell migration and invasion. Conversely, forced re-expression of miR-296 in highly invasive model breast cancer cell types suppressed tumor growth, in vivo.
Although previously implicated in VEGFR2- or PDGFRβ-signaling (Wurdinger et al., 2008), anti-viral mechanisms (Pedersen et al., 2007), retinoic acid-mediated differentiation (Houbaviy et al., 2003; Tay et al., 2008), or to prostate cancer growth and invasion (Wei et al., 2010), a role of miR-296 in cancer has remained controversial, with studies alternatively reporting increased expression (Hong et al., 2010), or, conversely, downregulation (Yang et al., 2009; Wei et al., 2010) in primary patient series. Here, miR-296 was almost universally downregulated in cancer, compared to matched normal tissues, and often lost in metastatic lesions. This had profound effects on the transcriptional profile of transformed cells, unrestraining a distinctive “miR-296-loss” gene signature, enriched in multiple key regulators of cell motility, invasion and metastasis. A recent report (Wei et al., 2010) showed that the oncofetal factor HMGA1 is a direct target of miR-296 in prostate cancer. In our system HMGA1 was significantly down-modulated at mRNA levels in miR-296 re-expressing cells (Figure 4b), though its protein levels were not affected by the miR-296 modulation (Supplementary Figure 5c). Conversely, one of these molecules over-expressed in the miR-296 signature was identified as the cell polarity-cell plasticity module, Scrib (Etienne-Manneville, 2008), which controls apical-basal cell polarity (Bilder et al., 2000), cell orientation (Osmani et al., 2006), and directional cell movements (Petrie et al., 2009) via the assembly of multi-protein complexes at the leading edge of migrating cells (Assemat et al., 2008).
Although these properties, coupled with the pro-tumorigenic phenotype associated with Scrib loss-of-function (Wu et al., 2010; Nagasaka et al., 2010), suggested a role in tumor suppression (Humbert et al., 2008; Wu et al., 2010, Ouyang et al., 2010), our findings point to a far more complex scenario for this pathway in human cancer (Gardiol et al., 2006). Here, Scrib was found abundantly over-expressed in disparate primary and metastatic epithelial malignancies, correlating with worse patient outcome, and mechanistically linked to aberrantly increased tumor cell motility and invasion. Other data also support a causal role of Scrib in human tumorigenesis, as over-expression of Scrib has been observed in colorectal cancer patients, correlating with accumulation of cytoplasmic β catenin (Kamei et al., 2007), the Scrib locus on 8q24.3 is often amplified in breast and ovarian cancer (Kim et al., 2007; Naylor et al., 2005), and Scrib was identified as a mediator of HCC progression, in vivo (Woo et al., 2009).
In this context, it is possible that Scrib may alternatively function in tumor suppression, or, conversely, tumor progression depending on the specific cellular context, and in particular, the complement of genetic alterations acquired during disease progression. For instance, Scrib may function to maintain apical-basal polarity, thus opposing tumorigenicity (Humbert et al., 2008; Wu et al., 2010) at early phases of cellular transformation, whereas more advanced disease stages, characterized by loss of multiple checkpoint/tumor suppressor mechanisms, may exploit aberrantly over-expressed Scrib (Osmani et al., 2006) to enhance random, as opposed to directional cell migration (Petrie et al., 2009), and thus gaining a critical advantage towards metastatic potential (Hanahan and Weinberg, 2000). It is also possible that the subcellular mislocalization of Scrib in the cytosol of tumor cells, as characterized here at variance with its distribution at cell-cell junction, may contribute to this diversity of functions, and promote aberrant cell migration and invasion. This is consistent with previous observations, in which over-expression of Scrib in astrocytes perturbed apical-basal polarity and promoted the formation of random actin protrusion during cell migration (Osmani et al., 2006).
In summary, we identified miR-296 as a global regulator of cell migration, invasion, and tumorigenicity, via direct transcriptional repression of a Scrib cell polarity-cell plasticity module (Etienne-Manneville, 2008). These results uncover a more complex scenario than previously thought for how cell polarity-cell plasticity modules may be exploited during human tumorigenesis (Humbert et al., 2008), whereas the identification of a miR-296-Scrib signaling axis in tumor cell motility (Petrie et al., 2009) may open new venues for the development of anti-metastatic therapies in humans.
All experiments involving animals were approved by an Institutional Animal Care and Use Committee. Pancreatic β cells were obtained by laser-assisted microdissection (LMD; Leica Microsystems, Milan, Italy) from total pancreas of four groups of RIP-TAg transgenic mice (two animals per time point) at the following stages of β cell tumorigenesis: normal/transgenic β cells (4-weeks of age), hyperplastic islets (6-weeks of age), angiogenic switch/carcinoma in situ islets (8-weeks of age) and invasive β cell carcinoma (10-weeks of age). Total pancreas was surgically isolated, formalin-fixed (10% buffered formalin) and paraffin embedded (FFPE). As controls, non-transgenic mice were sacrificed at the same age and processed as above.
Epithelial cells from matched normal colonic mucosa, dysplastic adenoma, adenocarcinoma or corresponding metastasis were isolated by LMD from FFPE blocks of 16 patients with diagnosis of colorectal carcinoma. Epithelial cells from non-neoplastic, tumor or metastatic tissue samples were similarly isolated by LMD from patients with diagnosis of adenocarcinoma of the breast (n=4), lung (n=4), stomach (n=9), bile ducts (n=2), or parathyroid tumors (n=1). Patients’ characteristics are summarized in Table 1. Total RNA was isolated using MasterPure RNA Purification Kit (Epicentre Biotechnologies, Madison, WI, USA) following the manufacturer’s instructions and quantified spectrophotometrically.
Total RNA and TMA blocks were available from a series of 62 cases of hepatocellular carcinoma (HCC). Patients’ associated clinical follow-up data was described previously (Augello et al., 2009). Informed consent was obtained from all patients, and the study was approved by an Institutional Review Board of the University of Milan, School of Medicine.
RT-PCR-based detection of 132 mature miRs and three mouse-specific reference snoRNAs (SNO 55, 412 and 142) was carried out from β cell samples isolated from RIP-TAg transgenic mice or control, non-transgenic mice using the microRNA Reverse Transcription Kit and gene-specific primers and probes (TaqMan MicroRNA Assays), according to the manufacturer’s specifications. All miRNAs were analyzed in duplicate, and instrument raw data (Ct values) were converted into miRNAs relative quantities (RQs) using the geometrical average of the three snoRNAs as normalization factor. For each miRNA, fold change ratios (FC) were calculated between 6, 8 and 10-week old RIP-TAg transgenic mice and 4-week old RIP-TAg animals. A FC=10 or 0.1 for over- or under-expression, respectively, was assigned as threshold for significant different expression. Significantly different miRs were analyzed in aged-matched non-transgenic mice as described above. The RNU48 was used as a reference snoRNA for human tissues or cell lines. For these experiments, miRNA expression relative to reference was calculated using the 2^(−ΔCt) formula. All reagents, primers, kits and instruments were obtained from Applied Biosystems (Life Technologies, Carlsbad, CA, USA).
Genomic DNA from tumor samples collected from 16 patients with diagnosis of metastatic colon adenocarcinoma was amplified with the following specific primers for k-Ras gene: k-Ras F: 5′-GTACTGGTGGAGTATTT-3′; k-Ras R: 5′-ATACAGCTAATTCAGAATCA-3′. Both strands of k-Ras amplicons were sequenced using BigDye terminators (Applied Biosystems, Life Technologies) and mutations occurring at codons 12 and 13 were identified.
Human colon carcinoma SW1116, hepatocellular carcinoma HepG2 and HUH-7, and breast adenocarcinoma MDA-MB231, MCF-7, SKBR3, and MDA-MB435 cells were purchased from the American Type Culture Collection (ATCC). Human embryonic kidney HEK293 cells were a generous gift from Dr. Locati (University of Milan). Normal human mammary epithelial cells (HMEC) were obtained from Gibco-Invitrogen (Life Technologies). Various cell types were seeded at 2×106 cells/well in 6-wells plates, and transfected with 100 pmol of pre-miR-296 (p-miR-296), antagomir-miR-296 (a-miR-296), pre-miR-1, pre-miR or Cy3-labeled anti-miR negative controls (Ambion, Life Technologies) in the presence of 5 μl Lipofectamine 2000 in 1 ml of OptiMem medium (Gibco-Invitrogen, Life Technologies). Stable miR-296 or control vector (GeneCopoeia, Rockville, MD, USA) expressing MDA-MB231 cells were generated after Lipofectamine 2000 transfection and puromycin (Sigma Aldrich, Milan, Italy) selection for one week. Then cells were trypsinized and plated without selection medium. MDA-MB231 with stable expression of miR-296 were validated by qPCR for recombinant miR expression and used for xenograft studies within passage four of culture.
Twelve female CD1 athymic mice were injected subcutaneously in the fourth mammary fat pad with 2×105 MDA-MB231 cells stably transfected with control miR or miR296 in a total volume of 100 μl of sterile PBS (six mice per condition). Tumor growth was monitored externally using vernier calipers and animals were euthanized after 3 weeks. Tumors were then formalin-fixed and paraffin embedded for histological examination. Tumor volume (mm3) was calculated using the formula: Volume = (width)2 × length/2.
MDA-MB231 cells were transfected with 100pmol of siGENOME or control Smart Pool siRNAs (cat. M-010500, D-001206 all from Dharmacon, Lafayette, CO, USA) and 5 μl of Lipofectamine 2000, as before. Subsequent to transfection, cells were maintained in complete medium for 24 or 48 and processed for individual experiments.
Cell cycle transitions and quantification of hypodiploid DNA content (i.e. sub-G1 cell fraction) were determined after 48 or 72 h in transfected cultures by propidium iodide staining and flow cytometry, as described (Romagnoli et al., 2008). Cells transfected with non-targeting constructs were used as unit sample.
MDA-MB231 or MCF-7 cells (5×103) were transfected with the various miRNA constructs, and seeded as a single-cell suspension in the presence of 1 ml of 0.7% top agar solution and 1% base agar solid layer after 48 h. Agar for both layers was dissolved in appropriate media supplemented with 10% FBS. Cell were cultured at 37°C, fed twice per week with complete culture medium, and plates were stained after 21 d with 0.5 ml of 0.05% Crystal Violet (Sigma-Aldrich) for 1h. Colonies with a diameter of at least 100 μm were counted by light microscopy and photographed.
We isolated tumor-associated fibroblasts from three patients surgically resected for breast cancer. Briefly the tissues were minced with blades and digested as previously described (Bauer et al., 2010). After isolation, CAFs were plated in cell culture dishes, cultured in 10%-FBS supplemented DMEM media (Gibco-Invitrogen, Life Technologies), and used for invasion assay of MDA-MB231 cells at the second and third splitting passage.
Subconfluent (70%) cultures of MCF-7, MDA-MB231 or HMEC cells were transfected with the various constructs for 24–48 h. Wounds in the cell monolayer were created using a P200 micropipette tip, after which cells were washed in PBS and incubated in complete medium for 24 h. For migration assay, three random images (50x) were taken at the time of the scratch and after 24 h. The migration distance (units) was determined as reduction in the wound’s gap using NIH Image-J software. For directional cell migration, subconfluent monolayers of MDA-MB231 cells were transfected with the various constructs, scratched as above after 66 h or 42 h, respectively, and analyzed for Golgi orientation after 6 h, by immunofluorescence. The position of the Golgi relative to the nucleus and to the migration front was scored using Image-J software in cells at the leading edge, as described (Dow et al., 2007; Osmani et al., 2006; Phua et al., 2009). Golgi staining was performed using Alexa Fluor555-conjugated antibody to GM130 (BD Bioscience, Milan, Italy). The direction of stress fibers was assessed in the same experiments. F-actin was imaged by phalloidin-TRITC staining (Sigma-Aldrich) using an AxioImager Z1 microscope (Carl Zeiss, Göttingen, Germany) were mounted in DAPI I (Abbott, Abbott Park, IL, USA).
MDA-MB231 or HMEC cells (5×104) transfected with the various constructs were seeded in serum-free medium in Matrigel-coated chambers (8.0 μm pores, BD Biosciences). Cells were allowed to migrate across coated inserts using serum-containing medium or CAFs as chemoattractant for 24 h. The cells on the apical surface of the insert were scraped off, and membranes with invaded cells were fixed in 100% methanol, stained with Toluidine blue (Sigma-Aldrich) and mounted on microscope slides. Invading cells were counted after photographing the membranes, and both the peripheral and the central areas were evaluated.
MCF-7 or MDA-MB231 cells were seeded (2×105) in poly-HEMA (20 mg/ml, Sigma-Aldrich)-coated 6-wells plates, after transfection with the various miRNA-mimics for 48 h or with the indicated siRNA for 24h. Cells were harvested after additional 24 h, and viability was assessed by propidium iodide content and flow cytometry (FACS). When PKH26 staining was performed (Sigma-Aldrich), 2×107 A549 or MDA-MB231 cells were labeled the day before transfection following manufacturer protocol.
The mRNA level of candidate genes (n=107, listed in Supplementary Table 1) was investigated in MDA-MB231 cells transfected with miR-296 or control constructs using TaqMan Gene Expression assays (Applied Biosystems, Life Technologies). TATA-binding protein (TBP) was used as housekeeping gene for target genes relative quantification (RQs) using the 2^(−ΔCt) formula. RQs were median-normalized and log2 transformed to generate an unsupervised hierarchical clustering. A 1.5 fold cutoff was used to select genes modulated by transfection of anti-miR-296 or pre-miR-296 relative to control, which were further analyzed using Ingenuity Pathway software. Functional profiling using Gene Ontology terms for biological process, molecular function and cellular component were conducted for miR-296 predicted targets identified by at least 4 algorithms (n=145) using GOTM tool (http://bioinfo.vanderbilt.edu/gotm). As reference gene set we used the human genome, and the top 10 functional categories (most significant p-values obtained using the hypergeometric test adjusted for multiple comparisons) with a minimum number of 4 required genes were identified (Supplementary Table 2).
Mutation in miR-296 seeding sequence within Scrib 3′UTR were created using QuikChangeII XL site directed mutagenesis kit (Stratagene, Agilent Technologies, Santa Clara, CA, USA). Vectors containing full length wild-type or mutated 3′UTR sequences of Scrib gene, or control sequence and dual luciferase reporter genes were purchased from GeneCopoeia. HEK293 cells were co-transfected as described above with 1 μg plasmid containing target gene 3′UTR or control sequence in the presence of 50 nM pre-miR-296, anti-miR-296, control oligonucleotides or unrelated miRNA constructs (anti-let-7g and pre-miR-1). Cells were lysed after 30 h and firefly to Renilla luciferase ratios was measured with a dual luciferase assay (Promega, Milan, Italy) using a Synergy 2 luminometer (BioTek, Winooski, VT, USA). Normalized luciferase ratios were determined for all combinations tested of miRNAs and vectors.
For immunoblotting, aliquots of MDA-MB231, MCF-7, or HMEC cells were harvested 48 or 72 h post-transfection, and solubilized in 150 μl of RIPA buffer supplemented with 1X complete protease inhibitor cocktail (Roche, Indianapolis, IN, USA). Cell lysates (50 μg) were separated by electrophoresis on 6% or 12% SDS-polyacrylamide gels, transferred to PVDF membranes (Millipore, Billerica, MA, USA), probed with 1 μg/μl of antibodies against Scrib (Santa Cruz Biotechnology, Santa Cruz, CA, USA), β-Actin (Sigma-Aldrich), BMP8A (Novus Biologicals Littleton, CO, USA), HMGA1 (LSBio Seattle, WA, USA) or cytokeratin AEI-AE3 (Dako, Milan, Italy), and reactive bands were visualized with ECL Plus reagents (GE Healthcare, Milan, Italy). CAFs were visualized by immunofluorescence staining with an antibody to vimentin (Dako). Immunohistochemical staining of FFPE tissue samples collected from patients with metastatic carcinomas or HCC, was carried out using an antibody to Scrib (10μg/μl, Santa Cruz Biotechnologies) for 1 h at 22°C followed by counterstaining with hematoxylin. As negative control, slides were incubated with dilution buffer instead of primary antibody. Slides were scored by light microscopy and photographed images were arranged with Photoshop for Windows. Cytoplasmatic and membranous Scrib immunoreactivity was scored as negative (0), weak (1), moderate (2) or strong (3) by two authors (GC and SB) independently.
All experiments were performed in duplicate and performed at least three times. Differences among samples were analyzed using Student’s t-test, unless otherwise specified. The correlation between k-ras mutation status and miR-296 in colorectal carcinoma patients was determined using the Fisher’s exact test. For survival analysis, the Kaplan–Meier method was used. To explore a potential association between miR expression and metastatic relapse, patients were assigned to two groups depending on miR-296 relative expression in tumor versus the averaged non-neoplastic counterparts. A miR-296 ratio of ≤0.5 was used for the “Low” group, whereas a miR-296 value of >0.5 was used for the “High” group. To estimate the association of Scrib mRNA or protein expression to tumor recurrence, HCCs patients were categorized in two groups according to Scrib expression value as for the miR. The two-sided log-rank test was used to compare survival curves. Statistical analyses were performed using GraphPad Prism version 4, or Ministat 2.1 software. A P<0.05 was considered as statistically significant.
Sources of Support for the present Investigation: This work was supported by grants from the Fondazione Invernizzi (to G.C.), Fondazione Berlucchi (to S.B.), and from National Institutes of Health grants HL54131, CA140043, CA78810 and CA118005 (to D.C.A).
We thank Riccardo Ghidoni, Michele Samaja and Massimo Locati for availability of laboratory equipment and reagents, Patrizia Doi and Delfina Tosi for technical help. A.F. is supported by a fellowship of the Doctorate School of Molecular Medicine at Università degli Studi di Milano.