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Guanylate-binding protein-1 (GBP-1) is an interferon inducible large GTPase involved in endothelial cell proliferation and invasion. In this report, expression and function of GBP-1 were investigated in vitro in intestinal epithelia after exposure to interferon-γ and in human colonic mucosa from individuals with inflammatory bowel disease (IBD). Interestingly, in contrast to other epithelia, GBP-1 distributed to the plasma membrane in intestinal epithelial cells where it colocalized with the tight junction protein coxsackie- and adenovirus receptor. In addition, expression of GBP-1 was upregulated in colonic epithelia of individuals with IBD. Downregulation of GBP-1 by siRNA resulted in enhanced permeability that correlated with increased apoptosis. Indeed, inhibition of caspase activity prevented the inhibition of barrier formation induced by the loss of GBP-1. These data suggest that GBP-1 is a novel marker of intestinal mucosal inflammation that may protect against epithelial apoptosis induced by inflammatory cytokines and subsequent loss of barrier function.
Guanylate-binding protein (GBP)-1 is one of the genes most strongly induced by interferons (IFNs).1 GBP-1 belongs to a family of GTPases which are classified into three groups: (1) the large GTPases, also known as GBPs; (2) the small GTPases; and (3) the Mx proteins.2 The human large GTPase family consists of seven members encoded by a gene cluster located on chromosome 1.3 The crystal structure of GBP-1 has revealed two different domains: a compact globular domain at the N terminus containing the GTPase function and an α-helical domain at the C terminus.4
GBP-1 is highly expressed in endothelial cells activated by inflammatory cytokines in vitro and in vivo and it regulates the inhibition of proliferation and invasion of endothelial cells in response to IFN-γ.5–7 GBP-1 has been shown to exert antiviral activity against vesicular stomatitis virus and encephalomyocarditis virus.8 Downregulation of GBP-1 by means of siRNA resulted in higher levels of hepatitis C virus replication.9 In addition to its GTPase function and its involvement in viral infections, GBP-1 also contributes to cell survival as overexpression of GBP-1 caused inhibition of apoptosis in human umbilical vein endothelial cells after growth factor and serum depletion.10 GBP-1 can be isoprenylated at a CaaX-motif at the very C-terminal end.4,11 Recently, it has been demonstrated in HeLa cells that overexpressed GBP-1 translocates to the Golgi membrane after IFN-γ stimulation. This translocation required nucleotide binding, isoprenylation, and IFN induction of the cells.12 However, despite the isoprenylation motif, GBP-1 has never been shown to be located at the plasma membrane.
Very little is known about GBP-1 expression and function in human epithelial cells.6,13 In epithelial cells, several groups have demonstrated that IFN-γ treatment can lead to apoptosis and compromised barrier function through different effects that may include sensitization to other inflammatory cytokines and/or FAS ligand.14–17 In intestinal mucosal tissue, chronic inflammatory conditions may manifest as inflammatory bowel disease (IBD), a chronic, relapsing disorder of the gastrointestinal tract.18,19 There are two major forms of IBD: Crohn’s disease (CD) and ulcerative colitis (UC), both of which lead to long-term, sometimes irreversible damage of the gastrointestinal structure and function. The pathogenesis of IBD is still poorly understood. However, it is known that multiple factors are implicated, such as genetic variations, altered gut flora, and a defective immuneregulation.18–21 Of note, IBD is characterized by mucosal tissue damage, apoptosis, and increased levels of proinflammatory cytokines such as the GBP-1-inducing interferons. Proinflammatory cytokines cause altered expression profiles in leukocytes and epithelial cells that affect the epithelial barrier.18 Genes regulated by inflammatory cytokines are therefore of great importance as targets for the development of new ideas for IBD treatment.
We hypothesized that GBP-1 may be induced under inflammatory conditions in intestinal epithelial cells and that it may be involved in regulating barrier function. We found increased GBP-1 levels in IFN-γ-treated human intestinal epithelial cells, in colonic mucosa of individuals with IBD, and we observed a localization of GBP-1 at tight junctions (TJs) exclusively in intestinal epithelia. In addition, GBP-1 downregulation by siRNA inhibited epithelial barrier formation due to a higher susceptibility to apoptosis under inflammatory conditions. The implications of these findings with respect to mucosal protective mechanisms are discussed.
Different human epithelial cell lines that were treated with 100 U/ml IFN-γ or untreated were screened for the expression of GBP-1 mRNA using intron-spanning primers to avoid amplification of genomic DNA. As a positive control, we used untreated and IFN-γ-treated 14-day-old human macrophages. By semiquantitative RT-PCR analyses, all cells tested showed an increase in GBP-1 mRNA level after IFN-γ treatment (Figure 1a). However, the strongest upregulation of message was observed in the cervical epithelial cell lines Caski and HeLa, and in the retinal epithelial cell line ARPE all of which expressed very low levels of GBP-1 mRNA in the resting state. By contrast, the intestinal epithelial cell lines T84, HT29, and SK-CO15 as well as human macrophages all exhibited detectable levels of GBP-1 mRNA in the untreated state and had variable increases in mRNA levels after IFN-γ treatment. The increase in message was most pronounced in T84 cells.
Next, GBP-1 protein expression was investigated by western blot (Figure 1b). Protein levels of GBP-1 were very low to absent in all untreated cells tested. After IFN-γ-treatment, there was a strong increase of GBP-1 protein in intestinal as well as in nonintestinal epithelial cells. However, we observed differences in mRNA and protein amounts especially in the resting state. Such discrepancies in the relative amounts of proteins and their mRNAs are difficult to explain, but certainly not unusual. Others have shown that only approximately 50% of observed changes at the protein level actually correlate with corresponding mRNA levels. The authors discuss such cases and give possible explanations.22
In subsequent functional studies, SK-CO15 cells were used as this transformed cell line forms high resistance, polarized monolayers, and is readily transfectable.23 Interestingly, SK-CO15 cells had the lowest amount of GBP-1. However, coincubation with IFN-γ and tumor necrosis factor (TNF)-α enhanced GBP-1 expression (Figure 1c), presumably due to TNF-α-induced enhancement of IFN-γ receptor expression.24 However, TN F-α alone did not induce GBP-1 expression.
The intracellular localization of GBP-1 was investigated using immunofluorescence (IF) staining and confocal laser microscopy. Human macrophages were used as positive controls and showed strong staining in the cytosol after IFN-γ treatment (Figure 2a). Untreated cervical epithelial cell lines HeLa and Caski showed no GBP-1 staining, whereas the untreated retinal epithelial cell line ARPE showed weak cytosolic staining (Figure 2a). After IFN-γ treatment, Caski and ARPE cells showed very strong cytosolic staining, whereas HeLa cells showed a lower amount of GBP-1 compared with the other cell lines (Figure 2a). The TJ molecule coxsackie- and adenovirus receptor (CAR) was stained to visualize the intercellular junctions. CAR belongs to the CTX family of transmembrane proteins and was originally identified as a virus receptor before its location at the TJ and its function as adhesion molecule were discovered.25 At the TJ, CAR has been shown to be involved in regulating epithelial barrier function and in homotypic intercellular interactions. No colocalization of GBP-1 and CAR could be detected in the above cell lines.
Intriguingly, the expression pattern of GBP-1 was strikingly different in intestinal epithelial cell lines. All three intestinal cell lines T84, SK-CO 15, and HT29 showed weak staining for GBP-1 in the resting state (Figure 2b). However, after IFN-γ treatment or IFN-γ + T NF-α for SK-CO15 cells, there was strong lateral membrane staining that colocalized with CAR (Figure 2b). In addition, the CAR expression did not seem to change in these cell lines after 24 h exposure to IFN-γ, as it was previously reported for endothelial cells.26 This finding was corroborated in xz images that also showed colocalization at TJs (Figure 2b). Such intercellular staining was unexpected, given that GBP-1 has not been previously reported to localize to the intercellular junctions.
To independently confirm the presence of GBP-1 at the plasma membrane, cell fractionation experiments were performed using T84 cells that were treated with IFN-γ (Figure 3a). The purity of subcellular fractions (membrane, nuclei, and cytosol) was assayed by western blot for specific marker proteins (Figure 3b). Aliquots of the total cell lysates before fractionation were probed for GBP-1 and demonstrated upregulation of GBP-1 protein levels after IFN-γ treatment. Nuclear fractions contained no GBP-1 protein. Western blots of cytosol fractions showed weak bands for GBP-1 in untreated cells and strong upregulation of protein expression after IFN-γ treatment. Of note, western blots of membrane fractions of IFN-γ-treated cells also showed strong GBP-1 expression (Figure 3a). These findings suggest that GBP-1 translocates from the cytosol to intercellular junctions under inflammatory conditions in intestinal epithelial cells.
As proinflammatory cytokines are elevated in mucosal tissues from individuals with IBD, we investigated whether GBP-1 is also upregulated in these tissues. IF staining revealed minimal GBP-1 expression in normal control tissue without signs of inflammation, whereas a strong upregulation of GBP-1 was observed in colonic epithelia of individuals with active UC (Figure 4). GBP-1 was also observed to be upregulated in mucosa of individuals with active CD but to a slightly lesser degree than in UC. We performed fluorescence pixel intensity analyses for each condition using LSM-FCS software (Zeiss, Jena, Germany) and obtained the following results (arbitrary units of pixel intensity): control tissue: 13.72 ± 4.94; UC: 72.63 ± 13.37; and CD: 50.36 ± 10.5. Compared with control GBP-1 staining, the increases in both UC and CD are highly significant with P-values of ≤ 0.001.
In a fashion similar to that observed in vitro, GBP-1 colocalized with CAR at the TJ in mucosal tissue samples of individuals with active CD and UC. By contrast, the small amount of GBP-1 detectable in control tissue was present in the cytosol only.
Given the colocalization of GBP-1 with intestinal epithelial TJs, we speculated that GBP-1 may be involved in regulating epithelial barrier function. To test this hypothesis, we employed a gene-silencing approach after 24 h of IFN-γ treatment with specific downregulation of GBP-1 by transient transfection with siRNA. The specificity of GBP-1 downregulation was demonstrated by western blot and IF staining (Figure 5a). Cells in which cyclophilin B (CyB), a gene not related to barrier function, was silenced served as controls. Transfection of SK-CO15 cells with GBP-1 siRNA resulted in a complete removal of GBP-1 from intercellular junctions (Figure 5a). The development of transepithelial electrical resistance (TER) was monitored every 24 h in mock-transfected cells and in cells transfected with CyB or GBP-1 siRNA. Development of TER was significantly impaired in cells transfected with GBP-1 siRNA compared with mock-transfected cells and cells transfected with CyB siRNA (Figure 5b). TER development of SK-CO15 cells after siRNAtransfection but without IFN-γ treatment has been previously reported by our group and showed a generally higher TER over time than the IFN-γ treated cells in the present study.23
As a complementary assessment of permeability, paracellular flux of 4 kDa fluorescein isothiocyanate-labeled dextran was measured in the same experimental setup. After transfection with GBP-1 siRNA and determination of effects on TER, dextran was added and flux measured 24 h later. As expected, greater than a twofold increase in paracellular flux was detected in cells transfected with GBP-1 siRNA compared with controls (Figure 5c). These findings support the notion that GBP-1 loss is detrimental to barrier function under inflammatory conditions.
In order to determine the mechanism of altered barrier function after GBP-1 knockdown, SK-CO15 cells were screened for signs of apoptosis after IFN-γ and GBP-1 or CyB siRNA treatment. Transfected cells were harvested when differences in TER were observed and probed for different apoptosis markers by western blot (Figure 6a). Tubulin blots served as loading controls. Apoptosis markers investigated were poly-(ADPribose)-polymerase (PARP), caspase-3, and caspase-9 as cleavage of these molecules is an early sign of apoptosis. PARP is a major target for cleavage by active caspase-3, which in turn is cleaved by caspase-9.27 The protein band for the large PARP-fragment (Δ-PARP) was enhanced in cells transfected with GBP-1 siRNA to a greater extent than in those transfected with CyB siRNA (Figure 6a). In addition, the proenzymes caspases 9 and 3 were cleaved, thus representing more activation in cells treated with GBP-1 siRNA (Figure 6a). Taken together, these findings indicate increased susceptibility to apoptosis after GBP-1 downregulation. To corroborate these findings, we performed terminal transferase dUTP nick-end labeling (TUNEL) staining (Figure 6b). SK-CO15 cells transfected with GBP-1 siRNA displayed stronger TUNEL labeling than those transfected with CyB siRNA. Quantification of labeled cells demonstrated more than a twofold increase in TUNEL labeling of cells transfected with GBP-1 siRNA compared with controls (Figure 6b). Addition of the caspase inhibitor Z-VAD to cells transfected with GBP-1 siRNAs protected these cells from apoptosis. In addition, IF staining for active caspase-3 was assessed and corroborated the TUNEL results (data not shown).
To determine whether caspase-mediated apoptosis is indeed a mechanism for altered barrier function, we performed TER measurements in cells transfected with GBP-1 or CyB siRNA that were additionally treated with the caspase inhibitor Z-VAD. Caspase inhibition reversed the impaired barrier function in cells transfected with GBP-1 siRNA. By contrast, control cells were unaffected by the addition of Z-VAD (Figure 6c).
The importance of GBP-1 in response to inflammatory stimuli has previously been studied by others in different cell types where expression of GBP-1 was induced by proinflammatory cytokines.1,6,13,28–30 In this study, we demonstrated expression of GBP-1 in cultured intestinal epithelial cells after exposure to IFN-γ and in colonic epithelia of individuals with IBD. Strikingly, an intestinal epithelial cell-specific association of GBP-1 with the lateral cell membrane and colocalization with the TJ marker CAR was observed. Importantly, loss of GBP-1 expression negatively affected the development of epithelial barrier function, presumably due to increased apoptosis induced by proinflammatory cytokines.
GBP-1 was detected at intestinal epithelial TJs and long-term treatment with IFN-γ has previously been shown to mediate intestinal epithelial barrier disruption in vitro and in vivo and also apoptosis possibly due to sensitization to other proinflammatory cytokines such as TNF-α.15,17,24 Thus, we speculated that GBP-1 expression under inflammatory conditions may initially be an epithelial response to maintain barrier function. Indeed, at least in vitro, GBP-1 protects epithelial barrier function by preventing apoptosis. However, the presence of GBP-1 at intercellular junctions in colonic mucosal tissue of individuals with IBD suggests that there are long-term compensatory mechanisms for GBP-1 expression in chronically inflamed states with altered barrier function. Whether GBP-1 has also a protective function in early stages of IBD remains to be investigated. A protective effect of GBP-1 may either be short-lived in IBD or, more likely, the negative, long-term effects of IFN-γ in IBD including the sensitization to TNF-α may outweigh the protective effect of GBP-1. Different functions of GBP-1 after either short- or long-term exposure to IFN-γ have also been observed by others in endothelial cells.10 Effects of GBP-1 expression after short-term exposure to IFN-γ resulted in decreased apoptosis. This finding is consistent with our data that GBP-1 loss after short-term treatment with IFN-γ causes decreased barrier function due to increased apoptosis. According to these findings, both IFN-γ and IFN-γ have comparable beneficial short-term effects. By contrast, long-term effects of IFN-γ treatment resulted in a senescent endothelial cell phenotype accompanied by reduced cell proliferation,10 which has also been observed by others.5 Although GBP-1 expression after short-term treatment with interferons seems beneficial to endothelial and also epithelial cell function, long-term exposure to interferons seems to be generally accompanied by decreased cell function and expression of GBP-1 is no longer protective.
Given the unique localization of GBP-1 at intercellular junctions of intestinal epithelial cells, it is likely that GBP-1 function may be different from that in other cell types in which GBP-1 expression is restricted to the cytosol. Thus, it is tempting to speculate that GBP-1 has tissue-specific functions. In particular, the intestinal epithelium is highly specialized with regard to barrier function and immune response to myriads of commensal and sometimes pathogenic microorganisms. For example, under hypoxic conditions, the intestinal epithelium has been shown to maintain barrier function in contrast to responses observed in other epithelia.31 Therefore, GBP-1 expression at TJs might be a factor exploited by intestinal epithelial cells to protect against pathophysiologic conditions. However, additional studies investigating GBP-1 function and expression in different organs under different conditions are required.
Recently, murine GBP-1 (mGBP-1) was identified as a major target gene in the interleukin (IL)-10 −/− model of mouse colitis on different genetic backgrounds (C3H/HeJ, C57BL/6J).32 The authors identified 20 genes as candidate genes by gene chip analyses, due to their location within a colitis-susceptible quantitative trait loci interval and function in the immune response. The authors reported that the effect of the genetic background on the expression levels was important for three genes, one of which was mGBP-1.32 In this context, three observations are important about mGBP-1: First, the mGBP-1 gene maps to the interval of the main colitogenic quantitative trait loci on mouse chromosome 3.32–34 Second, it is highly upregulated in IFN-γ-stimulated murine cells.35 Third, GBP-1 is already known to be polymorphic between different murine inbred strains: mGBP-1 is inducible in C3H/HeJ (colitis-susceptible) mice whereas it is not in C57BL/6J (colitis-resistant) mice.36 In addition, mGBP-1 has been shown to be induced in mice after infection with different microorganisms.37 The authors concluded that GBP-1 expression in this mouse model is part of the host defense mechanism as altered gut flora and microbial infection have also been shown to be involved during the pathogenesis of IBD.18 According to these findings in mouse models of colitis and to our finding that GBP-1 is localized at colonic epithelial TJs in individuals with IBD, we hypothesize that GBP-1 may be important in regulating intestinal epithelial barrier function in IBD.
In conclusion, our findings suggest that GBP-1 expression is an initial protective event against apoptosis induced by proinflammatory cytokines in intestinal epithelia. These findings open a new direction for understanding GBP-1 function and point to a critical role of GBP-1 in the response to intestinal mucosal inflammation. Thus, GBP-1 may be an important target gene for IBD therapies and other pathologic conditions with mucosal inflammation. The manipulation of GBP-1 expression or potential signaling mechanisms might be beneficial in early stages of acute inflammation before progression to a chronic-damaged state.
Human intestinal (T84, HT29), human retinal (ARPE-19), and human cervical epithelial cell lines (HeLa, CaSki) were obtained from ATCC (Manassas, VA) and cultured according to the provided protocols. The human intestinal epithelial cell line SK-CO15 was a gift from Dr Enrique Rodriguez-Boulan (Weill Medical College, Cornell University, NY) and cultured as described.38 During the last 24 h before harvesting, all cells were incubated in the presence or absence of 100 U/ml IFN-γ (+ 1 0 ng/ml TNF-γ (BD Biosciences, Franklin Lakes, NJ) for SK-CO15 cells).
Human monocytes were isolated from whole blood of healthy human volunteers using Ficoll/dextran sedimentation as previously described.39 The procedure for leukocyte isolation was approved by Emory’s Institutional Review Board. Human monocyte-derived macrophages were obtained as previously described by culturing 1.8×106 monocytes per six-well in RPMI 1640 (Sigma, St Louis, MO) containing 20 % human serum (Lonza, Walkersville, MD), 1% nonessential amino acids, 1% sodium pyruvate, and 0.1 mg/ml penicillin/streptomycin/L-glutamine (Sigma) for 14 days.40
Total RNA was isolated from cell lysates using the RNeasy Mini Kit (Qiagen, Valencia, CA). cDNA was synthesized by reverse transcription using oligo(dT12–18) primers and superscript II reverse transcriptase (Invitrogen, Carlsbad, CA). PCRs were performed using Taq-DNA polymerase (Roche, Indianapolis, IN). To avoid PCR amplification of genomic DNA, forward and reverse primers were located in different exons. Primer sequences were: GBP-1-FW: GGTCCAGTTGCTGAAAGAGC and GBP-1-RE: TGACAGGAAGGCTCTGGTCT. PCR conditions were: 95 °C for 5 min followed by 37 cycles of 95 °C for 15 s, 55 °C for 30 s, and 72 °C for 45 s followed by 72 °C for 10 min. PCR products were separated by agarose gel electrophoresis.
T84 cells treated with 100 U/ml IFN-γ for 24 h were washed in phosphate-buffered saline and equilibrated for 5 min at room temperature in buffer S (0.25 M sucrose, 1 mM imidazole, and 5 mM MgCl2). Cells were harvested in buffer S containing 1 mM dithiothreitol and a protease inhibitor cocktail (Sigma), incubated on ice for 15 min and then homogenized using a douncer. Cells were centrifuged at 800g at 4 °C. The supernatant was collected and the pellet of nuclei was washed three times with buffer N (10 mM Tris, 10 mM NaCl, 3 mM MgCl2, and 0.05 % NP-40, pH 7.4), vortexed for 30 s and centrifuged at 800g for 5 min. The washed nuclei were lysed with RIPA buffer (20 mM Tris, 150 mM NaCl, 2 mM EDTA, 2 mM ethylene glycol tetraacetic acid, 1 % Na+ deoxycholate, 1% Triton X-100, and 0.1% sodium dodecyl sulfate, pH 7.4) and sonicated. The supernatant containing membrane and cytosol fractions was centrifuged at 4 °C for 45 min at 100,000g. The supernatant (cytosolic fraction) was collected and the pellet (membrane fraction) was resuspended in a buffer containing 25 mM Tris, 150 mM NaCl, 1% NP-40, 4 mM EDTA, 25 mM sodium fluoride, and 1 mM sodium orthovanadate, pH 7.4 and then sonicated. Fractions were analyzed by immunoblotting. Purity of the fractions was controlled by western blots of marker proteins for each fraction: mouse anti-human β1-integrin as membrane marker (BD Biosciences), mouse anti-human GM130 (BD Biosciences) as Golgi marker and rabbit anti-promyelocytic leukemia protein as marker for the nuclear fraction (ABBiotec, San Diego, CA).
Equal amounts of protein were separated by polyacrylamide gel electrophoresis and transferred electrophoretically to polyvinylidene fluoride membranes. After incubation in phosphate-buffered saline containing 5 % skim milk for 1 h to block unspecific binding, the membranes were probed with rat anti-human GBP-1 antibody (clone 1B1; Calbiochem, La Jolla, CA) or mouse anti-α-tubulin (clone B-5-1-2; Sigma) as loading control for 1 h at 37 °C, washed three times in phosphate-buffered saline containing 0.5% skim milk and 0.05% Tween 20 and incubated with species-specific peroxidase-conjugated secondary antibodies (Jackson-Laboratories, Bar Harbor, ME) for 1 h at 37 °C. Signals were visualized using BM chemiluminescence substrate (Roche) and Hyblot ECL films (Denville, Metuchen, NJ).
Human epithelial cells were grown on glass cover slips in 24-well format to 70% confluency and then incubated for 24 h in the presence or absence of 100 U/ml IFN-γ (in case of SK-CO15 cells 100 U/ml IFN-γ + 1 0 ng/ml TNF-α). Cells were fixed for 20 min in ice-cold ethanol and blocked for 1 h in 1% BSA and 10% normal goat serum followed by incubation with anti-GBP-1 and mouse anti-CAR (clone RmcB, kind gift from Dr J Bergelson, Division of Infectious Diseases, Children’s Hospital of Philadelphia, PA) for 1h. Cells were washed and incubated for 1 h with species-specific fluorescently labeled Alexa-555 and Alexa-488 antibodies (Invitrogen). Cover slips were mounted in ProLong Gold medium (Invitrogen) and examined using an Axiovert LSM510 confocal laser microscope (Zeiss). For tissue staining, 8 µm frozen tissue sections were mounted on glass coverslips. Discarded human colon tissue samples (n = 3 for each condition: control, active UC, and active CD) were derived from anonymous surgical resection specimens or colonoscopy biopsies (active sites of UC and CD without extensive ulceration) and approved by the Emory University Institutional Review Board on human subjects. Sections were fixed in 100 % ethanol (−20 °C, 20 min) and air dried. Fluorescent labeling and analysis was performed as described above. In addition, nuclei were stained for 1 min using ToPro-3 dye (Invitrogen) after incubation with secondary antibodies. Fluorescence pixel intensities of GBP-1 labeling have been quantified by analysing 10 different fields of each condition using the LSM-FCS software (Zeiss).
SK-CO15 cells were grown to 50% confluence and then treated with IFN-γ and TNF-α. Gene knockdown41 was performed as described earlier23, using two different siRNAs (Qiagen): GBP-1_3, AAGGCATGTACCATAAGCTAA and GBP-1_6, ATGGCATGTACCATAAGCTA. A validated siRNA against CyB obtained from Dharmacon (Chicago, IL) served as control. Transfections were performed using HiPerfect (Qiagen) in OptiMEM I medium (Invitrogen) according to the manufacturer’s protocol.
SK-CO15 cells were plated on collagen-coated permeable polycarbonate transwell filters (Costar) with 0.4 µm pore size and 0.33 cm2 surface and grown to 50 % confluence. Cells were treated with IFN-γ and TNF-α for 24 h before siRNA transfection as described above. TER of epithelial monolayers was measured every 24 h using an EVOMX electrovoltmeter with an STX2 electrode (World Precision Instruments, Sarasota, FL). Six independent experiments in six filters each were performed.
SK-CO15 cells were prepared on transwell filters as described above. When differences in TER were measured (usually 3–4 days after transfection), monolayers were washed three times with Hanks’ balanced salt solution buffer before 10 µl of the tracer solution (10 µg/µl fluorescein isothiocyanate–dextran of 4kDa; Sigma) were added to the apical side of monolayers. After 24 h of incubation at 37 °C, media from the bottom chamber were collected and the amount of diffused dextran was measured in a fluorometer (excitation wavelength = 492 nm and emission wavelength = 520 nm).
SK-CO15 cells were transfected with siRNA to GBP-1 or CyB in transwell filters. Apoptosis was analyzed when differences in TER were observed. Cells were harvested in lysis buffer and apoptosis was detected by western blot using caspase-3, caspase-9, and PARP antibodies (Cell Signaling Technology, Danvers, MA). TUNEL staining was performed using TUNEL Label and TUNEL enzyme (Roche), according to the manufacturer’s instructions. The caspase inhibitor Z-VAD (Calbiochem) was applied at a final concentration of 10 µM where indicated with medium change after transfection and renewed every 24 h until changes in TER were observed. Quantification of TUNEL-labeled cells was performed using ImageJ.
Data are presented as the mean with standard error and were compared by Student’s t-test.
We thank Dr Susan Voss for expert cell culture, Moshe Bachar for technical assistance, Dr Jan-Michael Klapproth (Department of Gastroenterology, Emory University Hospital, Atlanta, GA) for providing tissue material, and Dr Jeffrey Bergelson (Division of Infectious Diseases, Children’s Hospital of Philadelphia, PA) for providing anti-CAR mAb RmcB. This work was supported by grants (RO1) DK72564, DK61379, and DK079392 from the National Institutes of Health to CAP and Schn 1155/1-1 from the German Research Foundation (DFG) to M.S.
The authors declared no conflict of interest.