1. University Hospital Heidelberg, Department of Gastroenterology, Im Neuenheimer Feld 410, 69120 Heidelberg, Germany;
2. University Hospital Regensburg, Department of Clinical Chemistry and Laboratory Medicine, Franz-Josef-Strauss-Allee 11, 93053 Regensburg, Germany.
Background and aims: The etiopathogenesis of inflammatory bowel diseases (IBD) remains largely unexplained. Flotillins (flotillin-1 and flotillin-2) are ubiquitous proteins which have been linked to inflammation and regeneration. We hypothesized that alterations in the expression of flotillin-2 in enterocytes may be related to the pathogenesis of IBD as a classical example of an inflammatory disorder of mostly unknown origin.
Methods: Cell and tissue localization of flotillin-2 (and -1) were investigated by immunofluorescent staining in 1. polarized and unpolarized CaCo-2w cells as a model of human enterocytes (native and after TNFα stimulation) and 2. intestinal biopsies from controls, patients with ulcerative colitis (UC) and patients with Crohn's disease (CD). For quantification of flotillin-2, we analyzed its expression in ileal and colonic biopsies from controls, UC patients and CD patients using real-time RT-PCR, Western blot and indirect immunofluorescence.
Results: In polarized CaCo-2w cells and human enterocytes in biopsies, flotillins were localized at the basolateral membrane and on subapical vesicles, but not in the apical membrane. Flotillin-2 expression did not differ between UC patients, CD patients and controls. However, it was significantly higher in colonic biopsies compared to ileal biopsies in all groups.
Conclusions: By virtue of its abundant expression in enterocytes, flotillin-2 must have an essential function in intestinal physiology, especially in the colon. Yet our data could not link flotillin-2 to the pathogenesis of IBD.
Keywords: Inflammatory bowel disease (IBD), Ulcerative colitis, Crohn's disease, Lipid raft, Flotillin-1, Flotillin-2.
Flotillin-1 (reggie-2) and flotillin-2 (reggie-1) are ubiquitous, highly conserved proteins that were first described to be upregulated in regenerating retinal ganglion cells of a goldfish.[1-3] Both flotillins were shown to be associated with lipid rafts and have been used as raft marker proteins. Flotillins are associated with the cytosolic side of the plasma membrane, but are also present intracellularly in different vesicular compartments like endosomes, lysosomes and phagolysosomes.[6-12] They appear to be expressed in all mammalian cells and tissues and possess a wide spectrum of functions in cell signaling, endocytosis, phagocytosis and interactions with the cytoskeleton.[5,13] However, there remain many open questions and controversies about flotillin function.
In mammals, flotillin-2 is widely expressed in numerous different tissues, while flotillin-1 appears to be more restricted. Flotillin-1 is highly expressed in brain, heart, placenta and hematopoietic cells.[15,16] In contrast, PCR analysis of flotillin-2 in murine and human tissues showed ubiquitous expression.
To date, several diseases have been described in which the expression of flotillins was distinctly altered. Among them are malignant tumors such as breast cancer, where flotillin-1 was found to be overexpressed in 61% of the samples examined. Flotillin-1 has also been demonstrated to be overexpressed in spinal cord cells of Lewis rats with experimentally induced autoimmune encephalitis as an example of inflammation. In a recently published manuscript, Song et al. showed that flotillin-1 was upregulated in esophageal squamous cell carcinoma (ESCC). It was demonstrated to activate TNFα receptor signaling and to sustain activation of NF-κB in ESCC cells.
The disease group of IBD comprises ulcerative colitis (UC) and Crohn's disease (CD). Both are chronic, non-infectious inflammatory diseases of the human intestine. Their etiopathogenesis still remains largely unknown. However, it is becoming clearer that a combination of an intestinal barrier dysfunction with an over-activated immune system might play a key role.
Why examine flotillins in IBD? Data are very scarce on flotillins in IBD so far; however, a few data are available on a potential role of lipid rafts in IBD.[22,23] Lipid rafts are abundant in enterocytes, especially in their apical cell membranes. Representing signal transduction platforms, lipid rafts are fundamental players in processes of inflammation and immunity. The effects of many mediators of inflammation which are considered to have roles in the pathogenesis of IBD - like interleukin-1β, TNFα, TRL2, CD14 und TLR4 - seem to depend on rafts.[26-28] Lipid rafts may also induce signal transduction processes that are necessary for the intrusion of pathogens into their target cells.[24,29,30] Pathological changes to lipid raft function might thus interfere with epithelial barrier integrity against intestinal bacteria. A link between alterations in lipid raft function in the intestinal tract and IBD may also be suggested due to the known therapeutic effects of phosphatidylcholine (PC), the latter seeming to interfere with raft composition and function and thus to alleviate inflammation.[31-33]
Unpublished microarray data obtained via Affymetrix U133 gene chip expression analysis of RNA samples from human intestinal biopsies suggest that flotillin-2 may have a role in IBD (method described in [34, 35]). They showed reduced flotillin-2 expression compared to controls in a limited number of biopsies taken from non-affected mucosal areas in patients suffering from UC. Even though flotillin-2 gene expression was predominantly low in the colon, it was also lower in ileum specimens from patients with ulcerative colitis compared to ileum specimens from controls.
Flotillin-2 as a player in regeneration, differentiation and inflammation, which are all essentially involved in IBD, thus appeared to be an interesting target for IBD research with the following primary objectives: 1. To localize the protein in vitro in native and TNFα-treated CaCo-2w cells, representing a model of human intestinal epithelial cells with or without inflammation; 2. To compare the results to in vivo localization data in human intestinal biopsies from controls and patients with UC or CD. 3. To analyze flotillin-2 expression in biopsies from healthy subjects and IBD patients at the RNA and, especially, protein level.
Caco-2w cells are a subclone of human Caco-2BBe cells with a well-differentiated phenotype (kindly provided by J. R. Turner, University of Chicago, IL). The cells were maintained under standard tissue culture conditions using Dulbecco's Modified Eagle's Medium (DMEM) supplemented with 4.5 g/L glucose, 10% heat-inactivated fetal calf serum, 2 mM glutamin, 0.1 mM non-essential amino acids, 1 mM sodium pyruvate and antibiotics (100 IU/ml streptomycin and 100 µg/ml penicillin). The cells were cultivated in plastic flasks at 37 °C under 5% CO2.
For polarization on semipermeable filters, Caco-2w cells were seeded in 6-well Vitaris transwell polyester membrane inserts (pore size 0.4 µm; Vitaris AG, Baar, Switzerland) and cultured for 2 to 3 weeks. TNFα (Promega, Madison, WI) was applied at 1 ng/ml or 2 ng/ml (1 h, 37 °C) on subconfluent Caco-2w cells.
All ileal and colonic biopsies were acquired endoscopically from patients visiting the Department of Endoscopy of the University Hospital Heidelberg. They were taken during colonoscopy and immediately transferred into liquid nitrogen, either as is or in RNAlaterTM for RT-PCR (Ambion, Frankfurt, Germany). Prior to examination they were stored at -80 °C. Since most proteins are differentially expressed within the colon, colon samples were taken from the transverse colon in all patients. In order to avoid gene expression influenced by inflammatory processes, biopsies were taken from non-inflamed mucosal areas or areas with as little macroscopic inflammation as possible.
Three groups of patients were examined: healthy controls, patients with UC, and patients with CD. Diagnoses of UC and CD were made on the basis of patient histories, endoscopic and histologic findings. These patients had different disease activities when they were examined. Controls were patients admitted for colonoscopy screening or undergoing colonoscopy for various abdominal complaints. None of the controls had a history of IBD, and in none of the controls did we find evidence of inflammation. Demographic and clinical characteristics of the subjects whose specimens were used for immunoblotting are shown in Table 1. As it would not add significant information, corresponding detailed clinical data of patients whose samples were used for PCR are not shown.
For Western blot analysis, we included altogether 32 ileal (11 controls, 11 CD patients and 10 UC patients) and 30 colonic biopsies (10 controls, 10 CD patients and 10 UC patients). RT-PCR analyses were performed from 72 biopsies (12 subjects in each of the three groups from the ileum and colon, respectively). The study was performed in accordance with the Declaration of Helsinki and approved by the local Ethics Committee.
Table 2 summarizes all the antibodies used in this study with their application, sources and dilutions. Antibodies against flotillin-1 were raised in rabbits according to standard procedures using a synthetic peptide (Sigma-Genosys, Cambridge, UK) coupled to keyhole limpet hemocyanin. The peptide corresponded to the C-terminus of human flotillin-1 and contained an additional N-terminal cysteine (CVNHNKPLRTA). Affinity purification of the antiserum was as recommended by the manufacturer on a peptide-agarose column (Pierce, Rockford, IL).
Characteristics of the patients whose biopsies were used for Western blot analysis. UC: ulcerative colitis; CD: Crohn's disease; f: female, m: male; y: yes, n: no; d.n.a.: does not apply. The term “active disease” was defined on the basis of colonoscopic and histologic findings.
|(neo-)terminal ileal manifestation (y/n)||d.n.a.||0/10||7/4||d.n.a.||1/9||9/1|
|colonic manifestation (y/n)||d.n.a.||10/0||9/2||d.n.a.||10/0||7/3|
|active disease (y/n)||d.n.a.||8/2||9/2||d.n.a.||9/1||10/0|
Sources and specifications of antibodies used in the study.
|CEA, A0115||h||rb||IF||DAKO, Glostrup, Denmark||1:400|
|Flotillin-1||h||rb||IF||provided by Kai Simons, Dresden, Germany||1:1000|
|Flotillin-2, 610383||h||m||IF, WB||BD Biosciences Pharmingen, Heidelberg, Germany||IF: 1:100|
|Na-K-ATPase, MA3-928||h||m||IF||ABR Affinity BioReagents, Golden, USA||1:50|
|ß-actin, A55441||h||m||IF, WB||Sigma-Aldrich, St Louis, USA||1:100,000|
|cy2 α-mouse, 715-225-151||m||d||IF||Jackson ImmunoResearch, West Grove, USA||1:230|
|cy2 α-rabbit, 711-225-152||rb||d||IF||Jackson ImmunoResearch, West Grove, USA||1:250|
|cy3 α-mouse, 715-165-151||m||d||IF||Jackson ImmunoResearch, West Grove, USA||1:1000|
|cy3 α-rabbit, 711-165-152||rb||d||IF||Jackson ImmunoResearch, West Grove, USA||1:1000|
|anti-mouse HRP, 115-035-003||m||g||WB||Jackson ImmunoResearch, West Grove, USA||1:5000|
h - human; m - mouse; rb - rabbit; d - donkey; g - goat; IF - immunofluorescence; WB - Western blot.
Immunofluorescence was used to localize flotillin-2 and flotillin-1 in cultured cells and human intestinal biopsies. For confocal microscopy, CEA and Na-K-ATPase were used as apical and basolateral membrane markers, respectively.
Cells grown on coverslips were washed twice with PBS and then fixed and permeabilized with ice-cold methanol for 2 min in -20 °C. Unspecific binding was blocked for 30 min at room temperature with PBS containing 0.01% saponin, 0.2% gelatin and 5 mg/ml BSA. Primary antibodies (see Table 2) in SGB solution were added for 1 h at room temperature. After primary antibody binding, the cells were washed 3 times with PBS containing 0.01% saponin and 0.2% gelatin.
The fluorescent-conjugated secondary antibodies (CyTM3 anti-mouse) were added for 1 h at room temperature. Subsequently, the cells were washed twice with SG solution, twice with PBS and once with water, and mounted on microscopic slides using Mowiol (Calbiochem, Bad Soden, Germany). The polarized Caco-2w cells on the filters were prepared as described above. For immunohistochemistry, frozen biopsies were embedded in Tissue Tek (Sakura Finetek, Zoeterwoude, NL) on dry ice. Five micron cryosections were prepared at 22 °C in a cryostat (model CM 3050S, Leica, Bensheim, Germany) and mounted on glass slides. Fixation and permeabilization were performed using acetone for 5 min and then methanol for 2 min, both at -20 °C. Slides were then blocked with 4% pig normal serum (DAKO, Glostrup, Denmark) in SGB solution for 30 min. Primary and secondary antibodies were applied as indicated above. In some experiments, Phalloidin Fluo Probes 547 (KMF Laborchemie, Lohmar, Germany) was added to the secondary antibody solution in a 1:10,000 dilution. Nuclei were stained with 1 µg/ml Hoechst 33342 (Roche, Mannheim, Germany).
All images of cultured cells and tissues except those from confocal microscopy were acquired on an Olympus IX50 fluorescence microscope using a 60 x oil immersion objective and analySIS software from Soft Imaging System (Muenster, Germany). Confocal microscopic images were obtained on a Leica TCS SP2 confocal microscope (Leica Microsystems, Wetzlar, Germany) using the HCX PL APO 63x1.32 oil objective. Images were arranged with Adobe Photoshop (Adobe Systems, Mountain View, CA).
For immunoblotting, proteins were extracted from intestinal biopsies. Each biopsy was transferred into a tube with 200 µl of sample buffer (125 mM Tris-HCl pH 6.8, 4% SDS, 20% glycerin), vortexed thoroughly and incubated at 95 °C for 5 min. After centrifugation, the supernatants were transferred to new tubes for protein determination using bicinchoninic acid (BCA). Equal amounts of protein (5 µg) were used from each subject. In order to optimize the comparability between patient groups and between different gels, the 12 lanes of each gel were loaded as follows: 3 to 4 control samples, 3 to 4 UC samples, 3 to 4 CD samples, 1 defined total Caco-2w cell lysate sample as well as a weight marker. The proteins were then separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) in 10% gels and transferred to nitrocellulose membranes. After transfer, the nitrocellulose sheets were stained with Ponceau S (Serva, Heidelberg, Germany) to visualize the protein bands. The membranes were subsequently incubated with anti-flotillin-2 (1:5000 in 2% skim milk) and anti-ß-actin (1:100,000 in 2% skim milk) overnight at 4 °C, followed by a 1 h incubation period with horseradish peroxidase-conjugated secondary antibody (1:5000 in 2% skim milk) at room temperature. After chemiluminescent detection with a commercial ECL reagent following the manufacturer's instructions (Amersham Biosciences, Buckinghamshire, UK), the films were scanned and bands were quantified by determination of density using MCIDTM Analysis Evaluation 7.0. For internal control, densitometry values obtained for flotillin-2 in every specimen were related to the value obtained for ß-actin from the same patient. For comparison, these values were related to the flotillin-2/ß-actin values in the total cell lysates.
For quantification of human flotillin-2 mRNA transcripts, total RNA was isolated from intestinal biopsies using the RNAqueous RNA isolation kit, and subsequently purified with the DNA-free kit (both from Ambion, Cambridgeshire, UK) according to the instructions of the manufacturer. Total RNA concentrations were determined photometrically at 260 nm. For each biopsy, a volume equivalent to 1 µg of total RNA was used for reverse transcription using the Transkriptor First Strand cDNA Synthesis Kit (Roche Diagnostics, Mannheim, Germany). Calibration plasmids containing the sequence of the human flotillin-2 gene were prepared as follows: DNA was isolated from CaCo-2w cells using the QIAamp DNA mini Kit (Qiagen, Hilden, Germany). The desired sequence was amplified by PCR using the Omniscript-RT Kit (Qiagen, Hilden, Germany). The amplified DNA fragment was purified by agarose gel electrophoresis. It was then inserted into the TA vector using the pGEMT vector ligation system (Promega, Mannheim, Germany). Vectors were subsequently transformed into E. coli, and plasmids were isolated from E. coli cultures with the NucleoSpin Plasmid Kit (Macherey-Nagel, Düren, Germany).
Real-time PCR was performed using the LightCycler 2.0 system (Roche, Mannheim, Germany). Transcripts were detected with SYBR Green I and normalized to human ß-actin. Flotillin-2/ß-actin ratios were calculated using Relative Quantification Software Version 1.0 und GIMP 2.2.
Primer sequences (5' to 3'): human flotillin-2 ACAGCTGAGGCCCAGTTG, TGAGCTCCTTGTCCGTACG; human ß-actin AGGATGCAGAAGGAGATCACTG, GGGTGTAACGCAACTAAGTCATAG.
Documentation, data processing and graphic presentation of results were performed using Apache OpenOffice Calc., SPSS version 15 (SPSS Inc., Chicago, IL) and GraphPad Prism 3.0 (GraphPad Inc., San Diego, CA). Data are presented as means and standard errors of the mean (SEM). Non-parametric Kruskal-Wallis with Dunn's post-test was used for comparisons between the 3 patient groups and the Mann-Whitney-U test for comparison of ileal vs. colonic biopsies. The level of significance was set at p ≤ 0.05.
Immunostaining revealed distinct flotillin-2 expression in the plasma membrane as well as in intracellular vesicular structures in unpolarized CaCo-2w cells (Figure 1A). The experiments on unpolarized CaCo-2w also showed that the localization of flotillin-2 was cell-cell contact dependent. Figure 1B demonstrates how cell-cell contacts caused increased expression of flotillin-2 in the area of the cell adjoining a neighboring cell. In parallel, we observed a reduction in flotillin-2 expression within intracellular vesicles.
In order to analyze the effects of cell differentiation on flotillin-2 localization, polarized CaCo-2w cell monolayers were grown on filters and examined by immunofluorescence. To allocate flotillin-2 to different cell membrane domains (apical versus basolateral), our intent was to co-localize flotillin-2 with Na-K-ATPase as a basolateral marker. As both available antibodies were monoclonal mouse antibodies, using the same secondary antibody for fluorescence detection would have made it impossible to discern between flotillin-2 and Na-K-ATPase. Therefore a flotillin-1 antibody (rabbit) was used for the basolateral co-localization studies. In unpolarized CaCo-2w cells and in a sample colonic biopsy, flotillin-1 and flotillin-2 co-localized almost completely (see Figure 2). Based on this close relation between flotillin-1 and flotillin-2, co-localization was also assumed in polarized CaCo-2w cells, so basolateral co-localization experiments were performed with flotillin-1 and Na-K-ATPase antibodies. Figure 3A displays co-localization of flotillin-1 and Na-K-ATPase in basolateral cell membranes of filter-grown polarized CaCo-2w cells. Flotillin-1 (and, correspondingly, flotillin-2) could not be identified within the apical plasma membrane and only barely within the basal plasma compartment, but were more evident within vesicle-like structures in the subapical cytoplasm (view Figure 3B).
(A) Immunofluorescence demonstrating the distribution of flotillin-2 in unpolarized CaCo-2w cells. Note that flotillin-2 is found in association with the plasma membrane and in intracellular vesicles. (B) shows that flotillin-2 localization in unpolarized CaCo-2w cells depends on cell-cell interactions. The CaCo-2w cells in the upper left of the image are in direct contact with neighboring cells. Accordingly, flotillin-2 is concentrated in their plasma membranes. The row of cells closest to the edge contains most of the flotillin-2 in cytoplasmic vesicles and only a small amount in the plasma membranes in close proximity to the neighboring cells on the left side. In the isolated cell in the bottom right of the image, flotillin-2 seems to be expressed only in cytoplasmic vesicles, but not in the plasma membrane.
(A) shows the co-localization (overlay yellow, on the right) of flotillin-2 (green) and flotillin-1 (red) in unpolarized CaCo-2w cells. (B) demonstrates the co-localization (overlay yellow, on the right) of flotillin-2 (red) and flotillin-1 (green) in a section of a human colonic biopsy.
(A) Polarized CaCo-2w cells with localization of flotillin-1 (red), Na-K-ATPase (green) and flotillin-1 and Na-K-ATPase immunofluorescence overlay (right). Flotillin-1 and Na-K-ATPase co-localize in the basolateral membrane. (B) Confocal microscopy image of polarized CaCo-2w cells. Flotillin-1 (red) is localized in a subapical compartment, but not in the apical membrane. Na-K- ATPase (green) marks the basolateral membrane.
As the major aim of the present study was to evaluate a potential role of flotillin-2 in the pathogenesis of IBD, an in vitro model of intestinal inflammation was used based on the hypothesis that expression and localization of flotillin-2 may be influenced by inflammation. However, treatment of CaCo-2w cells with TNFα for 1 h prior to fixation for immunofluorescence did not result in an altered localization of flotillin-2 within the cells (Figure 4). Based on this lack of change, the hypothesis was not pursued further in the present study.
Immunohistochemical analysis of human enterocytes in endoscopic biopsies from the ileum and colon revealed - as in the in vitro experiments - two reservoirs of flotillin-2: the cell membrane and intracellular vesicles. This is shown in exemplary biopsy cryosections, in which flotillin-2 localization was visualized in relation to enterocyte nuclei stained with Hoechst and the apical membrane markers CEA and actin (Figures 5A-D). Using confocal microscopy analysis and co-localization studies of flotillin-1 and the basolateral membrane marker Na-K-ATPase, we also found significant flotillin-1 enrichment in basolateral enterocyte membranes (Figure 6). As elaborated above, we suggest that these results could be translated to the localization of flotillin-2.
No shift in flotillin-2 expression (red) was noted in unpolarized CaCo-2w cells pretreated with TNFα at 1 ng/ml and 2 ng/ml for 1 h prior to fixation for immunostaining when compared to untreated cells (negative control).
Flotillin-2 is localized in subapical vesicles and in the basolateral membrane in human enterocytes. (A and B) Expression of flotillin-2 (red) in colonocytes in a human biopsy. Blue nuclear counterstaining was performed with Hoechst. Flotillin-2 accumulates in subapical vesicles. (C) shows flotillin-2 (red) in relation to CEA as an apical cell membrane marker (green). Note that there is no overlay. (D) shows flotillin-2 in green, actin stained by phalloidin in light red as an apical cell membrane marker and blue Hoechst counterstaining of nuclei.
Three-dimensional, confocal-microscopic images of a human colonic epithelial layer in a human endoscopic biopsy. Flotillin-1 is marked in red, Na-K-ATPase in green, immunofluorescence overlay on the right. Na-K-ATPase was used a marker of the basolateral cell membrane.
Three colonic biopsies and three ileal biopsies (3 controls, 3 UC patients and 3 CD patients) were analyzed by immunohistochemistry and compared to each another. For technical reasons, this evaluation focused on the subapical localization of flotillin-2. However, no difference was evident in the distribution pattern of flotillin-2 expression between IBD patients and the control subjects (images not shown).
Human intestinal tissue specimens were evaluated for their flotillin-2 expression by RT- PCR. In all, flotillin-2 expression was determined in 72 biopsies (3 x 12 from the ileum and the colon, 24 from controls, 24 from UC patients and 24 from CD patients). As shown in Figures 7A and B, flotillin-2 RNA expression levels did not show significant inter-group differences in either ileal or colonic biopsies (overall p = 0.98 for ileal biopsies, overall p = 0.43 for colonic biopsies). Comparative analyses of flotillin-2 RNA expression levels between ileal and colonic specimens revealed significantly higher expression in the colon than in the ileum, which proved true in all 3 patient groups (p < 0.0001 for controls, p = 0.009 for UC patients, p = 0.02 for CD patients).
A and B show levels of RNA expression in human ileal (A) and colonic (B) biopsies from 12 controls, 12 UC patients and 12 CD patients, respectively (one data point corresponds to one patient; means are indicated). Data were obtained using real-time RT- PCR. For internal standardization, flotillin-2 values were related to human ß-actin. Figure 7C displays results of flotillin-2 expression at the protein level, as achieved by Western blot analysis of protein extracts from ileal biopsies from 11 controls, 10 UC patients and 11 CD patients. Data points representing single patients and means are indicated. Figure 7D shows Western blot data from colonic biopsies from 10 controls, 10 UC patients and 10 CD patients. 7E and F show clippings from the three Western blot membranes used for analysis of flotillin-2 expression in ileal (E) and colonic biopsies (F), respectively (one number corresponds to one biopsy; a: Crohn's disease, b: control, c: ulcerative colitis; TLC: total cell lysate). The upper bands represent flotillin-2, the lower bands represent ß-actin.
At the translational level, real-time RT-PCR data were confirmed by immunoblot analysis. Sixty-two biopsies from the ileum and colon were analyzed in this way. Thirty biopsies originated from the colon (10 controls, 10 UC patients, 10 CD patients), and 32 biopsies from the ileum (11 controls, 10 UC patients, 11 CD patients) (Figures 7E and F). Regarding the ileal biopsies, relative densitometric values of flotillin-2 bands referenced to ß-actin bands and total cell lysate bands were 0.77 ± 0.19 in controls, 0.53 ± 0.04 in UC patients and 0.62 ± 0.07 in CD patients (overall p = 0.45) (Figure 7C). In the colonic biopsies, flotillin-2 expression likewise tended to be strongest in controls (1.42 ± 0.24) and slightly lower in patients with UC (1.10 ± 0.14) or CD (1.35 ± 0.20), without statistically significant intergroup differences (overall p = 0.62) (Figure 7D). However, underlining the results obtained by RT-PCR, Western blot analysis yielded significantly higher flotillin-2 expression in colonic biopsies when compared to biopsies acquired from the ileum (p = 0.01 for controls, p = 0.005 for UC patients, p = 0.02 for CD patients) (Figure 7). It was also of interest to correlate disease activity of IBD patients with flotillin-2 expression in their biopsies. Table 1 shows, though, that the vast majority of patients with UC and CD suffered from active disease when the specimens were obtained. Thus subgroups were too small for reasonable subgroup analysis. It is important to note, though, that the difference between flotillin-2 expression in the ileum as compared to that in the colon was smaller for CD patients than for UC patients. This might be due to the fact that most UC patients had active inflammation in the colon, but not in the terminal ileum. In contrast, 78% (7/9) of the patients with active CD at sample acquisition had not only colitis, but also ileitis (see Table 1).
This study was designed to investigate whether flotillin-2 might be involved in the pathogenesis of IBD, especially in that of UC. The hypothesis of a disease-prompting or disease-modifying role of potential alterations to the expression of flotillin-2 in the gut accrued from unpublished microarray data. These had revealed a reduced flotillin-2 RNA expression in biopsies from 4 UC patients when compared to controls.
In light of the data published by Kim et al., which showed an increased expression of flotillin-1 in autoimmune encephalitis, it seems at a first pass implausible to expect that the opposite, namely a reduced expression, of the related protein flotillin-2 may be a disease factor in UC. After all, UC has been considered to be a kind of autoimmune disease by some authors. However, taking into account the suggested functions of flotillin-2 in cells, such as regeneration, endocytosis and cell adhesion, any impairment of these by reduced flotillin-2 expression is indeed a factor to be considered as a potential initiator of inflammation, be it in the gut or elsewhere. Taking all of these facts together, it appeared intriguing to go further into this subject.
In order to test the hypothesis of a reduced flotillin-2 expression in the intestines of patients with UC, experiments were first conducted in vitro and then in vivo based on those findings. It was of foremost interest to ascertain whether the potential changes in flotillin-2 expression in UC and maybe also in CD could be reproduced at the protein level.
As we were interested in a potential role for flotillin-2 in IBD, we chose to use CaCo-2w cells as in vitro model first. The phenotype of CaCo-2w cells - albeit derived from human colon carcinoma - resembles more that of small intestinal cells than that of colon cells when grown on filters to attain polarization. We considered CaCo-2w cells, in both polarized and unpolarized states, to be an adequate model for our incipient in vitro experiments.
It is known that the expression of flotillins varies in different cell types and tissues.[13, 14] As in many other cell types in the human body, flotillin-2 was clearly expressed in CaCo-2w cells, being model cells of human enterocytes. There, flotillin-2 was distinctly found in association with the plasma membrane, but also to a high degree in association with intracellular vesicles. Interestingly, we observed a shift in flotillin-2 expression to areas of cell-cell contact and, in parallel, a reduction of flotillin-2 expression in intracellular vesicles. This is in agreement with previously reported findings by Stuermer et al. and Langhorst et al.[9, 38, 39] and underlines the suggested role of CaCo-2w cells in cell adhesion.
Immunofluorescence microscopy revealed co-localization of flotlillin-1 and flotillin-2 in CaCo-2w cells, supporting the notion that the two proteins can form hetero-oligomers. Accordingly, they have been observed together in other cells and tissues,[6, 40] supporting the idea that this mutual interaction also occurs in the gut. In undifferentiated CaCo-2w cells we found vesicles containing flotillin-1 (and 2) to be either diffusely scattered or concentrated in the perinuclear region. After polarization, however, expression of flotillins proved to be strictly confined to a subapical compartment. A similar phenomenon has been observed in T cells, in which both flotillins were found localized in “preformed caps”. Preformed caps are considered to be stable platforms with essential regulatory functions in T cell activation.[16, 41] These regulatory functions seem to mainly concern signal transduction and cytoskeleton dynamics. Therefore it may be concluded that flotillins also have an essential role in the differentiation of enterocytes, which are known for their high rate of cell turnover.
A novel and interesting finding of this study is that flotillin-1 (and -2), when looking only at the plasma membrane, seem to be confined to the basolateral compartment in polarized CaCo-2w cells, without appearance in the apical portion. Regarding this observation, we found no comparable data in the literature. The finding of a basolateral membrane compartmentalization of flotillins in enterocytes was confirmed in cryosections from human ileal and colonic biopsies. The absence of flotillins in the apical plasma membranes of enterocytes is striking, since flotillins are widely used as lipid raft markers, and lipid rafts are considered to be especially abundant in the apical cell membranes of enterocytes.[24, 25] Langhorst et al. have questioned the adequacy of flotillin-1 as a raft marker due to its prevailing intracellular localization. Based on the present data, it has to be considered once more whether flotillins can be employed as lipid raft markers in any cell line or tissue.
What does the basolateral localization of flotillins in enterocytes imply? The apical and basolateral poles of an epithelial cell have to meet rather different requirements. Major tasks of the basolateral cell membrane are reception and conversion of signals for proliferation, differentiation, migration and apoptosis. The apical pole, in contrast, mainly serves in absorption of nutrients and protection against aggressive external factors like acid, digestive enzymes and pathogens. We speculate that the basolateral localization of flotillins in enterocytes is associated with signal transduction and cytoskeletal dynamics, while the subapical, flotillin-containing vesicles are involved in endocytosis.
Knowing that flotillin-2, in line with the above-mentioned microarray data, is expressed in human enterocytes of the ileum and colon, we proceeded to a simple cell model of colitis to screen whether flotillin-2 expression was strongly influenced by pro-inflammatory signals. It was shown previously in the same laboratory that TNFα, added to the medium of sub-confluent CaCo-2w cells, leads to a time-dependent, efficient nuclear translocation of the p65 subunit of NF-κB as soon as 15 min after addition of TNFα. TNFα levels have been demonstrated to be increased in the intestinal mucosa from patients with CD and UC, and mucosal cultures from patients with the two diseases proved to produce more TNFα, IL-1β, and IL-6 compared to normal mucosa. In addition, anti-TNFα antibodies are used successfully in the treatment of IBD. Furthermore, lipid rafts, with which flotillins are considered to be associated, play a role in the activation of the NFκB cascade via TNFα activation. However, immunostaining of TNFα-stimulated CaCo-2w cells as compared to untreated cells did not show obvious differences in intracellular flotillin-2 localization. Of course these are no quantitative data. This experiment was interesting for another reason: Numerous phenomena have been published as potential actors in the pathogenesis of IBD. Many of them could not be clearly determined to be primary pathogenetic factors. For them, the chicken-or-egg question remains largely unanswered: does an alteration precede and thus cause inflammation, or does inflammation cause the alteration?
The TNFα data mentioned above could suggest that the exact sampling site of biopsies in the inflamed colon in the present study is not of great importance. Still, we sought to avoid biopsy collection from severely inflamed tissue, even though areas with slight or only microscopically visible inflammation were included.
In contrast to the above-mentioned microarray data showing a 5-fold reduction in flotillin-2 expression in UC patients, flotillin-2 expression in the human intestine had indeed a tendency to be lower in UC patients compared to healthy subjects, but no significant inter-group difference was established. This was not only the case at the RNA level but, more importantly, likewise at the protein level, as shown by immunoblotting. Since sample numbers were higher in this study and as expression analyses were also performed at the protein level, we believe that the present results outweigh the previous microarray data. Thus, our data do not imply a major role for flotillin-2 in the pathogenesis of IBD, even though they do not exclude a role of flotillin-2 in IBD for certain. A limiting factor is that sample numbers were small and the distribution of disease activities in the IBD groups was inhomogeneous. In view of the role of flotillin-2 in regenerative processes it might be worthwhile investigating its expression during the recovery phase induced by medication in order to exclude a role of flotillin-2 in IBD for certain. IBD patients included in our study suffered from UC or CD in equal numbers. The specimens represented a variety of different disease activities. The fact that macroscopically unaffected mucosal areas were preferred for sampling does not rule out the possibility that the measured flotillin-2 expression might have been influenced by inflammation in some cases. In future experiments, it might be interesting to take biopsies from inflamed and non-inflamed areas in the same patient.
The stronger expression of flotillin-2 in the colon compared to the ileum, even in healthy subjects, is remarkable and raises the question as to whether flotillin-2 possesses a special function in the colon. Major functions of the colon are absorption of water and electrolytes, while the ileum is mainly responsible for the absorption of vitamin B12, bile acids and remaining products of digestion entering from the jejunum. However, the colon and the ileum, the latter being mechanically separated from the cecum via the ileocecal valve, also differ greatly in the amounts of bacteria populating their lumina. The colon contains ca. 1011 to 1012 CFU/mL stool, whereas the ileum has bacterial concentrations of about 104 to107 CFU/mL stool. Yet our data are not sufficient to imply a role of flotillin-2 in defense of the host against intestinal bacteria. However, this could be an interesting starting point for further research, notably as we found flotillin-2 within the basolateral cell membranes of enterocytes, which are not in direct contact with bacteria.
Flotillin-2 is distinctly expressed in human enterocytes, where it concentrates at the basolateral plasma membrane and in subapical compartments, but interestingly not at the apical plasma membrane. This might imply that in the intestine its main function relates to cytoskeleton dynamics and signal transduction, as well as endocytosis. Its higher expression in the colon as compared to the ileum may indicate that flotillin-2 has an especially important role in the colon.
Our hypothesis of a reduced flotillin-2 expression in IBD - mainly ulcerative colitis - versus controls could not be confirmed by the present data, which were acquired at the level of RNA as well as protein. Thus, these findings do not suggest a major role for flotillin-2 specific to the pathogenesis of IBD, even though the sample numbers were small.
BCA bicinchoninic acid, CD Crohn's disease, CEA carcinoembryonic antigen, CFU colony forming unit, ESCC esophageal squamous cell carcinoma, IBD inflammatory bowel disease, PCR polymerase chain reaction, PFA paraformaldehyde, RT reverse transcriptase, UC ulcerative colitis.
We thank Sabine Tuma, Karin Bents and Richard Sparla for expert technical support. This publication contains parts of the medical thesis of Inga Buchholz. We thank Kai Simons (MPI Dresden, Germany) for providing flotillin-1 antibodies and Jerrold R. Turner (University of Chicago, IL) for providing Caco-2w cells.
The authors have declared that no competing interest exists.
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Corresponding author: Robert Ehehalt, M.D., University Hospital Heidelberg, INF 410, 69120 Heidelberg, Germany; E-mail: Robert.ehehaltuni-heidelberg.de.