Clusterin expression can be modulated by changes in TCF1-mediated Wnt signaling
© Schepeler et al. 2007
Received: 02 March 2007
Accepted: 16 July 2007
Published: 16 July 2007
Clusterin (CLU) is an enigmatic molecule associated with various physiological processes and disease states. Different modes of cellular stress lead to increased CLU levels, and additionally numerous growth factors and cytokines affect the expression of the CLU gene. APC and c-MYC, both intimately linked to the Wnt signaling pathway have previously been shown to influence CLU levels, and we therefore investigated if changes in Wnt signaling activity in vitro could regulate the expression of one, or more, of several CLU mRNA and protein variants.
Over-expression of the cytoplasmic domain of E-cadherin tagged with GFP was used to abrogate Wnt signaling activity in LS174T and HCT116 colon carcinoma cells. This fusion construct sequestered signaling competent β-catenin whereby Wnt signaling was abrogated, and consequently cytoplasmic CLU protein levels increased as demonstrated by immunofluorescence. To determine which branch of the Wnt pathway was mediating the CLU response, we over-expressed dominant negative (dn) TCF1 and TCF4 transcription factors in stably transfected LS174T cells. We observed both intra- and extracellular levels of CLU protein to be induced by dnTCF1 but not dnTCF4. Subsequent analysis of the expression levels of three CLU mRNA variants by real time RT-PCR revealed only one CLU mRNA variant to be responsive to dnTCF1 over-expression. 5'-end RACE indicated that this CLU mRNA variant was shorter at the 5'-end than previously reported, and accordingly the translated protein was predicted to be shorter at the N-terminus and destined to the secretory pathway which fit our observations. Examination of the immediate expression kinetics of CLU after dnTCF1 over-expression using real time RT-PCR indicated that CLU might be a secondary Wnt target.
In conclusion, we have demonstrated that the Wnt signaling pathway specifically regulates one out of three CLU mRNA variants via TCF1. This CLU transcript is shorter at the 5' end than reported by the RefSeq database, and produces the intracellular 60 kDa CLU protein isoform which is secreted as a ~80 kDa protein after post-translational processing.
The clusterin (CLU) protein was first discovered more than 25 years ago in rat testis fluid because of its ability to facilitate clustering of a variety of cell types in culture. Since then, homologues of the broadly expressed CLU gene have been identified in several species and CLU proteins have been found in most mammalian body fluids. CLU is an enigmatic molecule, implicated in diverse biological processes, and has additionally been associated with opposing functions in regard to apoptosis. Accumulating evidence from several studies suggests that the pro- and antiapoptotic functions may be related to nuclear and secreted protein isoforms, respectively. The secreted form of CLU is a glycosylated protein of 70–80 kDa that consists of two chains held together by five disulfide bonds, and consequently it appears as a ~40 kDa smear on immunoblots from reducing SDS-PAGE. Its intracellular pre-curser form of 60 kDa may also exhibit an antiapoptotic function. The proapoptotic CLU variant is a 50–55 kDa protein which accumulates in the nucleus of apoptotic cells. How these different CLU protein variants are produced from the CLU gene is poorly understood, although it has been speculated that nuclear CLU results from an alternative splice event skipping exon 2 from the main CLU transcript otherwise translated into secreted CLU.
CLU is recognized as being a stress-inducible gene, thus responding to a variety of general stress stimuli such as oxidative stress, ionizing radiation and heatshock. In addition, several cytokines and growth factors either promote or suppress CLU expression in vitro. Numerous functional cis-elements and trans-factors have been identified which are responsible for regulating CLU expression under different conditions in vitro. Trans-factors which have been shown to interact with the CLU promoter, and regulate its activity, include Egr-1, members from the AP-1 complex, HSF1/2, Cdx1/2, and B-MYB. Hence, many cis/trans-factors have been identified which may be responsible for the complex tissue-specific control of the gene. The complexity of CLU regulation is also illustrated by the observations that identical growth factors may elicit different CLU responses depending on the cell type of exposed cells, and whether cells are grown as mono- or mixed cultures in vitro. In contrast to the avian CLU gene whose expression can be driven by two alternative promoters, CLU expression in mammals has traditionally been thought to be controlled by one promoter only. However, several novel CLU mRNA variants have recently been identified in human colon and prostate cells, and two of these transcripts were demonstrated to be differentially regulated by androgens in prostate cells[12, 13]. Considering the recent discovery of these CLU transcripts little is known about their biological relevance and regulation, including whether transcription of each mRNA species is initiated from the same promoter or perhaps different promoters. Furthermore, it is also unclear how they each relate to the different CLU isoforms observed at the protein level. Investigating these issues is important for understanding CLU regulation and function. Over-expression of oncogenes B-MYB and c-MYC, has been reported to induce and repress CLU, respectively[10, 14]. Of note, c-MYC is recognized as being a target of the Wnt signaling pathway. Another Wnt component, APC, lead to elevated CLU levels when being over-expressed in a null APC-/- human colon cancer cell line. Collectively, these studies made us speculate that one, or more, of the CLU mRNA variants might be regulated by Wnt signaling. Accordingly, we used a model system based on human colon adenocarcinoma cells to investigate whether CLU expression could be regulated by changes in Wnt signaling. Indeed, we show that by abrogating the otherwise constitutively activated Wnt pathway in these cells, CLU protein levels are up-regulated. Concomitantly, we observed increased levels of one out of three CLU mRNA variants, previously identified in colonic tissue. Induction of CLU is further demonstrated to be mediated by the transcription factor, TCF1.
Sequestration of β-catenin increases CLU protein levels in colon carcinoma cells
To determine if Clusterin protein levels are affected by alterations in Wnt signaling activity, we transiently transfected the colon carcinoma cell lines, LS174T and HCT116, with a fusion construct consisting of GFP fused to the cytoplasmic domain of E-cadherin. The encoded fusion protein efficiently sequesters signaling competent β-catenin, thus abrogating the Wnt signaling pathway which is otherwise constitutively activated in these cell lines due to activating mutations in β-catenin.
Altogether the data showed that inhibition of Wnt signaling by sequestration of β-catenin led to increased CLU levels.
Wnt regulation of CLU is mediated by TCF1
Wnt signaling regulates the secreted CLU protein isoform
The 60 kDa CLU isoform can be converted to a ~80 kDa heterodimer isoform through glycosylation and proteolytic cleavage. Consequently, this mature CLU isoform appears as a ~40 kDa smear on reducing SDS-PAGE immunoblots[2, 3]. In contrast to the cytoplasmic 60 kDa form, this latter CLU protein species is secreted by the cells and can thus be found in the extracellular milieu. However, under certain stress conditions, CLU can be diverted from its normal secretory pathway and reach the cytosol by means of retrotranslocatio. To investigate whether the CLU species induced by abrogated Wnt signaling was indeed secreted, western blotting was used to detect secreted CLU proteins in the culture medium at various time points after induction of dnTCF1. Our analysis revealed that CLU accumulated in the culture medium after induction of dnTCF1 (Fig. 3C). This was not the case for control cells. This implies that the up-regulation of the intracellular pre-curser form of CLU, 60 kDa, is followed by maturation and secretion of the mature CLU form. Accordingly, secreted CLU appeared as a ~40 kDa smear on the immunoblots. Not much, if any, of the ~40 kDa smear band was observed to accumulate intracellularly (Fig. 3A). This may be explained by a high secretion rate of CLU, which would keep the intracellular pool of mature CLU protein low, and has been observed to occur rapidly in human liver carcinoma cells (HepG2) with half-times of 30–35 min[17, 19].
dnTCF over-expression increase cell death rate in LS174T cells
Characterization of the 5' end of the NM_001831.2 mRNA variant
In silico analysis of CLU mRNA variants
Using the largest open reading frame (ORF), we predicted the CLU34 and CLU35 mRNA isoforms to produce identical proteins of 449 amino acids (AAs). In contrast, the CLU36 transcript produces a hypothetical protein of 460 AAs. The subcellular localization of these proteins was predicted to be nuclear in the case of CLU36, whereas the proteins produced from the CLU34/35 transcripts were secreted. Of notice, had CLU34 shared its 5' end with the NM_001831.2 RefSeq variant then a predicted nuclear protein of 501 AAs would be produced with expected distinct biological functions.
To summarize, the in silico predictions suggested that CLU34 and CLU35 might, individually or in combination, be responsible for the generation of cytoplasmic and secreted CLU proteins.
TCF1-mediated Wnt signaling specifically regulates the CLU34 mRNA variant
To determine if any of these CLU mRNA species was responsive to alterations in Wnt signaling, in which case they would be likely templates for the production of the 60 kDa/~40 kDa CLU proteins, we quantified the relative expression levels of each mRNA variant by real time RT-PCR at various time points after induction of dnTCF1.
To verify that these transcriptional responses were specific for dnTCF1, and not dnTCF4, we used real time RT-PCR to measure the expression levels of each CLU mRNA variant in response to dnTCF4 over-expression. As expected, none of the CLU mRNA variants responded to the induction of dnTCF4 (Fig. 7), and in agreement with our previous observations both CLU35 and CLU36 were expressed at very low levels, often below the detection limit of the real time RT-PCR assay (data not shown). Thus, CLU34 is specifically regulated by TCF1 in LS174T cells. In addition, over-expression of both dnTCF1 and dnTCF4 lead to a marked reduction of c-MYC mRNA levels which is consistent with c-MYC also being down-regulated at the protein level (Fig. 2D). Also, in agreement with previous reports, p21CIP1/WAF1 mRNA levels increased as a consequence of abrogated Wnt signaling by either dnTCF.
To investigate whether the extremely low expression levels of CLU35 and CLU36 were a characteristic unique to our model system, we screened a large panel of cell lines for baseline expression levels of these transcripts. Besides a variety of colon carcinoma cell lines, we also included a number of prostate carcinoma cell lines in our analysis since CLU has been reported to be up-regulated in this cancer type[24, 25]. In all 21 cell lines investigated, including LS174T and HCT116, both CLU35 and CLU36 were expressed at very low levels (see Additional file 2). In several cell lines the transcripts were expressed below the detection limit of the real time RT-PCR assay, and their expression levels did not correlate with that of CLU34 which was expressed at varying levels across the entire panel of cell lines (see Additional file 2). It therefore appears as if the expression of the CLU35 and CLU36 transcripts are regulated by a promoter different from the promoter controlling CLU34 expression, and that the former is only minimally activated and may require specific signals such as androgens to get stimulated. This notion fits the observation that CLU35 can be specifically up-regulated by androgens and that the responsive elements are located within the first 1200 bp of the CLU35 transcriptional initiation site. This genomic region is located approximately 2000 bp downstream from the CLU34 promoter/initiation site (Fig. 5).
Expression kinetics of CLU34 in response to over-expression of dnTCF1
While the expression of direct Wnt target genes is activated by binding of TCF transcription factors to specific sequence motifs in their promoters, the expression of indirect target genes are regulated via transcription regulators, which are targets of the Wnt pathway. For example, the direct Wnt target gene c-MYC, represses the expression of the indirect target p21CIP1/WAF1 by binding to the transcriptional activator MIZ1 at the p21CIP1/WAF1 promoter.
To get an indication of whether CLU was a direct or indirect Wnt target, we searched the genomic DNA sequences upstream of each unique CLU exon 1 for TCF binding motives as these would be a prerequisite for direct regulation of CLU by the Wnt pathway. Our analysis using the MatInspector software revealed a cluster of four potential TCF binding sites upstream of exon 1a (CLU34). Two additional potential TCF binding sites were localized downstream from exon 1a in the DNA region spanning exon 1a and exon 1c (Fig. 5A).
We used real time RT-PCR to see if the transcriptional response of the secondary Wnt target, p21CIP1/WAF1, matched that of CLU. This was indeed the case as p21CIP1/WAF1 mRNA levels did not increase markedly until 12 hr after addition of doxycycline (Fig. 8B). In conclusion, these data points towards CLU as being a secondary target of the Wnt signaling branch mediated by TCF1 although the specific trans-factors responsible for CLU induction remain to be experimentally identified in future studies.
Here, we demonstrate that abrogation of the Wnt signaling pathway in colon carcinoma cells lead to up-regulation of CLU. By further dissecting the molecular signaling cascade responsible for increased CLU levels, we find that changes in CLU expression are specifically controlled by the branch of the Wnt pathway mediated by the transcription factor TCF1.
Our finding, that CLU expression can be regulated by the Wnt signaling pathway, add to the plethora of stimuli which can regulate CLU levels. The CLU promoter has already been shown to be responsive to a variety of external stress-inducing agents such as oxidative stress, ionizing radiation, heat shock, and chemotherapeutics. In addition several types of growth factors including TGF-β, NGF, EGF, PDGF, βFGF, and interleukin-1,-2 and -6 have been demonstrated to influence CLU expression in cultured cells. Although some of these signals may ultimately converge on identical downstream effectors directly responsible for regulating CLU promoter activity, several unique trans- and cis-factors have been demonstrated to influence CLU levels[2, 3]. Thus, CLU expression can be modulated by many factors and their impact on CLU levels may in some cases be context dependent. For example, TGF-β and EGF treatment elevate CLU levels in some cell types whereas the very same growth factors suppress CLU expression in others. Also, interleukin-6 induced CLU expression in hepatoma cells (HepG2) whereas CLU was down-regulated in rat glial cultures exposed to the same cytokine[27, 28].
The Wnt signaling pathway is known to be involved in the development of colorectal cancer and is also of major importance in colon physiology. In particular, this pathway controls the maintenance of colon tissue architecture by controlling epithelial cell behaviour in the crypts of Lieberkühn. The pathway is activated in epithelial cells at the crypt bottom and decreases in a gradient toward the crypt top. In colonic epithelial cells, it may therefore be expected that CLU is expressed in an inverse pattern to that of Wnt signaling. This, however, does not seem to be the case in the adult human colon as it has previously been reported that CLU only stains a small fraction of scattered colonic epithelial cells with neuroendocrine differentiation. In this tissue it therefore appears as if the Wnt pathway is not the dominant force controlling CLU expression. Rather, CLU expression is likely the result of a complicated interplay between various pathways. The notion that the complexity of CLU regulation in vivo is not always being fully recapitulated by in vitro model systems, was also recently emphasized by Patel et. al who unexpectedly observed decreased CLU levels with rat donor age in glial cultures, despite CLU in vivo shows an opposite adult age trend: CLU expression increases during aging in select brain regions and in neurodegenerative disorders. Although Wnt signaling may not be the primary regulator of CLU expression in human colonic epithelial cells, other studies indicate that this might be the case in epithelia of the murine intestine. Lars E. French and colleagues used in situ hybridization (ISH) to investigate CLU expression during murine embryogenesis, and found CLU to be weakly expressed in dividing epithelial cells at the base of the villi in the small intestine but strongly expressed in more differentiated cells that line the rest of the villus. Similarly, Suh E. and colleagues used immunohistochemistry (IHC) to show that epithelia of the developing murine intestine was positive for CLU protein staining, and exhibited a gradient of activity with higher expression in the villus compartment than in the crypts. At least in the developing murine small intestine, it may therefore be that Wnt signaling contributes to modulate CLU expression in epithelial cells.
Although we identified which TCF factor was responsible for CLU up-regulation, namely TCF1, it remains to be demonstrated whether TCF1, or other downstream effectors, bind directly to the CLU promoter and regulate its activity. A previous study reported the Wnt target, c-MYC, to repress CLU expression in murine colonocytes although no direct interaction between c-MYC and the CLU promoter was demonstrated. In agreement with these observations we observed a decrease in c-MYC levels before CLU was induced upon over-expression of dnTCF1 in LS174T cells. However, considering that c-MYC levels also dropped when we over-expressed dnTCF4 and CLU levels remained unchanged, we do not believe c-MYC to regulate CLU levels in our model system. Notably, other investigators found no changes in CLU levels in murine fibroblast cells stably transfected with a c-MYC construct compared to mock transfected cells. Therefore, other factors might be more likely to regulate CLU in our model system, possibly, AP-1 or Egr-1 transcription factors which can bind directly to the CLU promoter[6, 7] and have been demonstrated to be suppressed by Wnt signaling.
It has become clear that the CLU gene encode several mRNA variants. At least three CLU mRNA variants are expressed in colon tissue, CLU34, CLU35, and CLU36. It has previously been reported that only one of these variants, CLU35, was down-regulated in human colorectal tumors samples compared to normal tissue indicating that the CLU mRNA variants may be differentially regulated. This view was supported by a recent study by Cochrane et al. who used real time PCR to demonstrate that two CLU transcripts could be differentially regulated in prostate cells by androgens. Interestingly, our results indicate that the Wnt signaling pathway, via TCF1, specifically regulate the expression levels of CLU34. Our 5'-end RACE results indicate that the NM_001831.2 sequence is not present in colon carcinoma cells and this observation is further supported by the failure to detect the full NM_001831.2 sequence by RT-PCR in normal and cancerous colon tissue samples. Instead, both RT-PCR and real time PCR can successfully detect a transcript, CLU34, which is shorter at the 5'-end and matches the most predominant CLU mRNA isoform previously reported[21, 2]. This shorter sequence has implications for the nature of the predicted protein because the ATG of the RefSeq NM_001831.2 exon 1 is not part of the CLU34 transcript and consequently the ORF of the predicted protein starts in exon 2. Hence identical proteins are predicted from the CLU35 and CLU34 transcripts. Importantly, this common protein is predicted to be secreted which fits exactly with what we find in our model system, as concomitantly with the induction of CLU34 mRNA an abrupt increase in cytoplasmic and secreted CLU protein species is observed. Thus, the CLU34 mRNA species apparently produce these protein variants.
The existence of two human CLU transcripts (CLU34/35) probably encoding identical CLU proteins is paralleled by previous findings in quail which demonstrated that two CLU transcripts with different, mutually exclusive, non-coding 5' exons can be produced from the avian gene. However, whereas the avian CLU transcripts are produced from two promoters often being co-regulated as suggested by correlating expression levels of the two CLU transcripts in tissue samples from a variety of organs, the human CLU transcripts are clearly differentially regulated.
In conclusion, we have demonstrated that the Wnt signaling pathway specifically regulates one out of three CLU mRNA variants via TCF1. This CLU transcript is shorter at the 5' end than reported by the RefSeq database, and produces the intracellular 60 kDa CLU protein isoform which is secreted as a ~80 kDa protein after post-translational processing.
Cell culture and transient transfections
LS174T derived and HCT116 cell lines were maintained in RPMI 1640 + 25 mM hepes medium (Invitrogen/Gibco, Carlsbad, CA, USA) and McCoy's 5A medium, respectively. Each medium was supplemented with 5% foetal bovine serum (Invitrogen/Gibco) and 1% penicillin-streptomycin (Invitrogen/Gibco).
The inducible LS174T derived cell lines have previously been described and were a kind gift from Dr. Hans Clevers (The Hubrecht Laboratory, The Netherlands). Induction was performed using 1 μg/ml doxycycline (Invitrogen). Selection was performed on all the LS174T derived cell lines using 10 μg/ml blasticidin (Invitrogen). 500 μg/ml zeocin (Invitrogen) was additionally used for inducible LS174T dnTCF1/4 cell lines. All cell lines were free of mycoplasma contamination as verified by the MycoSensor™ PCR assay kit (Stratagene, La Jolla, CA, USA) according to manufacturers instructions.
For transient transfection experiments involving immunofluorescence, LS174T and HCT116 colon carcinoma cell lines were transfected using Fugene 6 (Roche Applied Science, Hvidovre, DK), according to the instructions of the supplier. For transient transfection experiments involving western blotting, LS174T cells were resuspended at 2 × 106 cells/transfection in Amaxa buffer (solution V) and electroporated (program T30) with 10 μg of DNA per construct as per manufacturer's protocol (Amaxa, Cologne, Germany) and grown in 6-well plates. The GFP-cyt-E-cadherin plasmid was a kind gift from Dr. Philippe Blache (Institut de Génétique Humaine, Centre National de la Recherche Scientifique, France) and has previously been described. The GFP control plasmid, kindly provided by ph.d Sanne Harder Olesen, was a pcDNA3.1 vector harboring the EGFP gene excised from the pEGFP-N1 vector (Clontech).
Cell death assays
Two cell death assays, based on either trypan blue or propidium iodide (PI; Invitrogen) and hoechst 342 (HST; Invitrogen), were used to assess cell death rate in LS174T dnTCF1 and control cell lines 24 and 48 hr after induction. In brief, preattached cells were induced, and total number of cells (floating and attached) were pelleted. Cells were resuspended in either trypan blue solution (Sigma-Aldrich A/S, Copenhagen, Denmark) or a PBS solution containing DNA intercalating dyes, PI (10 μg/ml) and HST (20 μg/ml), and aliquots were transferred to a haemocytometer. For the trypan blue dye exclusion assay, cells were observed under a light microscope, and the extent of cell death was calculated as the percentage of stained cells (apoptotic and/or necrotic) relative to total cell number. For the PI/HST assay, images of stained nuclei were captured using a camera with appropriate filters mounted on a conventional fluorescence microscope. Viable cells were identified by intact nuclei with blue HST fluorescence and necrotic/apoptotic cells (permeable to PI) were identified by red PI fluorescence. To define a fixed area, accompanying white light (phase) pictures revealing the haemocytometer grid were layered on top of the fluorescence pictures in Adobe Photoshop software. An unpaired student's t-test was used to determine significant differences. Both assays were performed in biological triplicates.
Proliferation and viability assays
Proliferation rate of uninduced and induced LS174T derived cell lines were determined qualitatively by staining cultured cells with methyl violet (Bie & Berntsen, Rødovre, DK) after 5 days and quantitatively by manually counting attached cells in a haemocytometer after 4 days. Both assays were done in biological triplicates. Images of cells stained by methyl violet were acquired using a regular flatbed scanner after washing cells twice in PBS.
Cell viability was assessed using the Cell Proliferation Kit I (MTT) from Sigma-Aldrich according to manufacturers instructions. LS174T dnTCF1 and control cell lines were cultured in 96-well plates in medium with or without doxycycline. After 48 hours, absorbance of solubilized MTT formazan crystals was measured on a microplatereader (Labsystems Multiscan® MCC/340) at 540 nm. Experiments were done in quaduplicates.
5'end rapid amplification of cDNA ends
5'-end RACE was performed using the Marathon-Ready™ colon adenocarcinoma cDNA library (Clontech) according to the manufacturers recommendations. 5'-end RACE products were generated using an antisense CLU gene specific 5'-RACE primer complementary to part of CLU exon 3: 5'- GGCATCCTCTTTCTTCTTCTTGGCTTC-3'. The Marathon RACE PCR reaction was performed with Advantage 2 Polymerase Mix (50×) (Clontech). PCR products were gel purified using the QIAquick Gel Extraction Kit (Qiagen), and cloned using the TOPO TA Cloning® Kit for Sequencing (Invitrogen) according to the manufacturers instructions. Cloned products from three colonies were sequenced using Expand High Fidelity PCR System (Roche Applied Science) and BigDye Terminator Kit (Applied Biosystems) with an ABI 3100 Genetic Analyzer (Applied Biosystems). The following plasmid specific internal primers were used for sequencing; 5'-TAATACGACTCACTATAGGG-3' (sense) and 5'-CAGGAAACAGCTATGAC-3' (reverse)
Whole cell extracts were prepared; pelleted cells were lysed on ice in a lysis buffer containing 50 mM Tris, pH 7.5, 150 mM NaCl, 1% NP-40, 0.5% deoxycholic acid supplemented with protease inhibitor cocktail (Roche Applied Science). Analysis of CLU levels in the culture medium was done by acetone precipitation of the proteins in the culture medium, after which the pellet was resuspended in lysis buffer. Protein concentrations were determined by the Bradford assay. Samples were boiled 3 min in loading buffer (350 mM Tris HCL, 30% glycerol, 0.1% SDS, 600 mM DTT, 0.012% W/V bromophenol blue) prior to loading an equal amount of protein (20 μg cell extract, 40 μg from medium) on each lane on precast NuPAGE 12% Bis-Tris Gel (Invitrogen). Electrophoresis and blotting onto polyvinylidene fluoride (PVDF) membrane were performed according to standard minigel procedures for the Novex XCell II Mini-Cell system. All-Blue prestained standards (Bio-Rad) were used as molecular weight markers. After blocking with 3% skimmed milk, membrane was incubated with primary antibodies; mouse monoclonal anti-CLU (1:400; clone 41D; Upstate, Charlottesville, VA, USA), mouse monoclonal anti-c-Myc (1:100; clone 9E10; Santa Cruz Biotechnology, Santa Cruz, CA, USA), mouse monoclonal anti-TCF-1 (1 μg/ml; clone 7H3; Upstate), and mouse monoclonal anti-TCF-4 (1 μg/ml; clone 6H5-2; Upstate). Final protein detection used the secondary HRP-conjugated polyclonal goat anti-mouse antibody (1:2500; DakoCytomation) in combination with ECL Plus reagent (Amersham Biosciences). As loading control, parallel immunoblotting using an anti-β-actin mouse monoclonal antibody (0.05 μg/ml; clone AC-15; Sigma-Aldrich) was performed.
For immunofluorescence analysis, cells were cultured on glass coverslips. Cells were washed with PBS, fixed with 4% paraformaldehyde for 10 min at RT after which fixation was quenched by incubating in 0.1 M glycine-PBS solution for 5 min. Cells were permeabilized for 5 min with 0.1% Triton X-100 in PBS, washed with PBS, and blocked with 1% BSA in PBS for 45 min at 37°C. After washing with PBS, cells were incubated with primary antibodies, mouse monoclonal anti-CLU (1:400; clone 41D; Upstate) and mouse monoclonal anti-β-catenin (1:200; BD Transduction Laboratories), followed by another wash with PBS and then incubated with secondary antibody, AlexaFlour 546 goat anti-mouse IgG1 (1:400; Molecular Probes Inc.), for 1 h at 37°C. After being washed with PBS, nuclei was stained using DAPI (4,6-diamidino-2-phenylindole) (Sigma-Aldrich Denmark A/S, Copenhagen, DK), and cells were mounted on microscope slides and images were captured using a CCD camera (Quantix, Photometrics, Tucson, AZ, USA) mounted on a Leica DMRXA epifluorescence microscope (Leica, Wetzlar, Germany) with appropriate filters and operated via SmartCapture software (Digital Scientific, Cambridge, UK).
Real time RT-PCR
Quantitative real time RT-PCR was performed on an ABI PRISM® 7000 Sequence Detection System (Applied Biosystems, Foster City, CA, USA) using the relevant (TaqMan or SYBR Green) Master Mix (Applied Biosystems). For normalization, the gene Ubiquitin C (UBC) was used using primer sequences previously published. Total RNA was purified using the GenElute™ Mammalian total RNA miniprep kit (Sigma-Aldrich), including on-column DNase digestion (Qiagen). RNA integrity was evaluated by Bioanalyzer analysis using nano chips (Agilent Technologies). cDNA was generated using the Superscript™ cDNA synthesis kit (Invitrogen) with random nonamer primers and RNAse inhibitor (Ambion, Austin, TX, USA). The individual CLU mRNA variants were quantified using variant specific primer/probe sets previously reported. Each measurement was performed in triplicate, and no-template controls were included for each assay. Relative expression values were obtained using a four-point 10-fold dilution curve. The dilution curve was created using a cDNA pool containing 2 μl of each of the test cDNAs.
Sequencing of the genomic CLU locus
The integrity of the genomic CLU locus was analyzed by bi-directional sequencing using the BigDye Terminator Kit (Applied Biosystems) and the ABI 3100 genetic analyzer (Applied Biosystems). Fragments representing each exon and the adjacent intron-exon boundaries were generated by PCR. Primer details of the sense and antisense primers have been published elsewhere. Sequencing covered all 11 exons (Fig. 5A,B; 1a, 1b, 1c, and 2–9).
We would like to thank ph.d Karina Dalsgaard Sørensen and ph.d Sanne Harder Olesen for providing total RNA from various prostate and colon cancer cell lines. Dr. Philippe Blache for providing the GFP-cyt-E-cadherin plasmid. Dr. Hans Clevers for providing stably transfected LS174T cell lines. This work was supported by funds from the Danish Research Council, the Lily Benthine Lunds Fond, the Desiree og Niels Ydes Fond, the Aase og Einar Danielsens Fond, the King Christian X's Fond, and the John and Birthe Meyer Foundation.
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