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Open Access Highly Accessed Research article

TNF-α-induced up-regulation of pro-inflammatory cytokines is reduced by phosphatidylcholine in intestinal epithelial cells

Irina Treede1, Annika Braun1, Petia Jeliaskova1, Thomas Giese2, Joachim Füllekrug1, Gareth Griffiths3, Wolfgang Stremmel1 and Robert Ehehalt1*

Author Affiliations

1 Department of Gastroenterology, University of Heidelberg, INF 345, 69120 Heidelberg, Germany

2 Institute of Immunology, University of Heidelberg, INF 305, 69120 Heidelberg, Germany

3 Cell Biology Program, EMBL, Postfach 102209, 69117 Heidelberg, Germany

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BMC Gastroenterology 2009, 9:53  doi:10.1186/1471-230X-9-53

The electronic version of this article is the complete one and can be found online at: http://www.biomedcentral.com/1471-230X/9/53


Received:26 July 2008
Accepted:13 July 2009
Published:13 July 2009

© 2009 Treede et al; licensee BioMed Central Ltd.

This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Background

Phosphatidylcholine (PC) is a major lipid of the gastrointestinal mucus layer. We recently showed that mucus from patients suffering from ulcerative colitis has low levels of PC. Clinical studies reveal that the therapeutic addition of PC to the colonic mucus using slow release preparations is beneficial. The positive role of PC in this disease is still unclear; however, we have recently shown that PC has an intrinsic anti-inflammatory property. It could be demonstrated that the exogenous application of PC inhibits membrane-dependent actin assembly and TNF-α-induced nuclear NF-κB activation. We investigate here in more detail the hypothesis that the exogenous application of PC has anti-inflammatory properties.

Methods

PC species with different fatty acid side chains were applied to differentiated and non-differentiated Caco-2 cells treated with TNF-α to induce a pro-inflammatory response. We analysed TNF-α-induced NF-κB-activation via the transient expression of a NF-κB-luciferase reporter system. Pro-inflammatory gene transcription was detected with the help of a quantitative real time (RT)-PCR analysis. We assessed the binding of TNF-α to its receptor by FACS and analysed lipid rafts by isolating detergent resistant membranes (DRMs).

Results

The exogenous addition of all PC species tested significantly inhibited TNF-α-induced pro-inflammatory signalling. The expression levels of IL-8, ICAM-1, IP-10, MCP-1, TNF-α and MMP-1 were significantly reduced after PC pre-treatment for at least two hours. The effect was comparable to the inhibition of NF-kB by the NF-kB inhibitor SN 50 and was not due to a reduced binding of TNF-α to its receptor or a decreased surface expression of TNF-α receptors. PC was also effective when applied to the apical side of polarised Caco-2 cultures if cells were stimulated from the basolateral side. PC treatment changed the compartmentation of the TNF-α-receptors 1 and 2 to DRMs.

Conclusion

PC induces a prolonged inhibition of TNF-α-induced pro-inflammatory signalling. This inhibition may be caused by a shift of the TNF-α receptors at the surface to lipid rafts. Our results may offer a potential molecular explanation for the positive role of PC seen in clinical studies for the treatment of ulcerative colitis.

Background

Inflammatory bowel disease (IBD) is the result of a chronic intestinal inflammatory response. While the exact pathogenesis of IBD remains incompletely understood, it is likely that the initiation of the immune response is triggered by luminal factors [1]. The nature of these initiating agents is unclear, but both orally ingested nutrients and microbial agents have been implicated [2]. It is widely believed that an impaired barrier function, and in particular a defect of the mucus layer, leads to an increased exposure of the mucosal immune system to luminal antigens. In genetically susceptible individuals, this results in an inappropriate and unrestrained inflammatory response [3,4].

We have recently shown that both PC and lysophosphatidylcholine (LPC) but neither phosphatidylethanolamine (PE) nor sphingomyelin (SM) are decreased in the mucus of patients with ulcerative colitis (UC) and that the oral substitution of PC using slow release preparations is beneficial [5-7]. How luminal PC influences the clinical course of UC is not yet known, but two scenarios are possible. First, because of its hydrophobic property, PC coats the mucus layer, thereby preventing the contact of luminal bacteria to the mucosa [5,8,9]. With respect to this, luminal PC has been shown to synergize with conjugated primary bile salts in the binding of luminal endotoxin, which in turn leads to a suppressed inflammation beyond the mucosal surface [10]. On the other hand, we could recently demonstrate that PC per se has anti-inflammatory properties. PC has been shown to inhibit membrane-dependent actin assembly and TNF-α-induced MAPkinase and NF-κB activation [11]. In light of these results, we hypothesized that luminal PC might be integrated into the plasma membranes of enterocytes and in turn modulate the signalling state of the mucosa in the human intestine. This assumption is further substantiated by studies using an in vitro phagosome system [12,13] which show that exogenous PC is indeed involved in the networks which inhibit pro-inflammatory signalling in membranes.

IBD encompasses two chronic intestinal diseases, Crohn's disease (CD) and UC, which differ in their microscopic and macroscopic features although their symptoms are similar [14]. Ulcerative lesions in IBD are accompanied by a prominent infiltrate of inflammatory cells including T lymphocytes, macrophages, neutrophils, and mast and plasma cells [15]. Mechanisms involved in the recruiting and activating of these inflammatory cells are thought to encompass a complex interplay of inflammatory mediators. This is reflected by the elevation of various chemokines in the serum and mucosa of IBD patients (for review see [16]). Over 40 human chemokines are now acknowledged, each with its own specific pattern of cellular chemotaxis. The chemokine family is categorised into four groups depending on the spacing of their first two cysteine residues [17]. Cumulative studies demonstrate that all four types of chemokines are involved in the development of IBD [16]. The expression level of pro-inflammatory chemokines differed significantly between IBD patients and controls. Up-regulated chemokine expression in human biopsies correlated with increasing activity of the disease [16]. Pro-inflammatory cytokines such as TNF-α and interleukin 1β (IL-1β) up-regulate the transcription of chemokine genes and hence the synthesis of chemokines themselves through the activation of NF-κB [18,19]. As TNF-α has been shown to be an important player in the inflammatory process of IBD [20], we previously established a model cell system with human intestinal epithelial cells (Caco-2) which we stimulated with TNF-α to induce a pro-inflammatory response [11]. Using this system, we now analysed the effect of various PC species on the transcriptional levels of selected marker genes. After PC treatment, the TNF-α induced up-regulation was significantly reduced in a time- and dose-dependent manner depending on the fatty acid composition. PC was effective when applied to the apical side of polarized Caco-2 cells if they were stimulated from the basal side. We could show that the TNF-α effect was dependent on NF-κB activity and not due to inhibition of the binding of TNF-α to its receptor. PC treatment changed the compartmentation of TNF-α-R1 and TNF-α-R2 to lipid rafts, which is a possible mechanism of action.

Methods

Lipids and reagents

TNF-α was obtained from Promega (Mannheim, Germany) and dissolved in endotoxin-free water containing 1% BSA from Sigma (Deisenhofen, Germany). Aliquots of 10 μg/ml were stored at -70°C. The NF-κB inhibitor SN 50 was from Calbiochem (San Diego, USA). PC 18:2/18:2 (1,2-dilinoleoyl-glycero-3-PC), PC 16:0/16:0 (1,2-dipalmitoyl-glycero-3-PC), PC 16:0/18:2 (1-palmitoyl-2-linoleoyl-glycero-3-PC), LPC 16:0 (1-palmitoyl-glycero-3-PC), PE 16:1/16:1 (1,2-dioleyl-glycerol-3-PE) were from Sigma (Deisenhofen).

Cells and bacteria

Caco-2w cells are a sub-clone of the human Caco-2BBe and were selected because of their well-differentiated phenotype. They were provided by J. R. Turner (University of Chicago). Cells were grown at 37°C and 5% CO2 in Dulbecco's modified Eagle's medium (DMEM) supplemented with 10% heat-inactivated fetal calf serum, 1% non-essential amino acid, and antibiotics (55 IU/mL penicillin and 55 μg/mL streptomycin). Vero cells (American Type Culture Collection; ATCC) were propagated in Dulbecco's Modified Eagle's Medium (DMEM) supplemented with 5% fetal bovine serum and antibiotics (55 IU/mL penicillin and 55 μg/mL streptomycin). For full polarization cells were grown for 14 d on 2.5 cm, 0.4 μm pore size Transwell polycarbonate filters (Costar, Cambridge, USA) as previously described [21].

Gene expression analyses by RT-PCR quantification

Caco-2 cells were grown under standard conditions in 6-wells for 48 h to 90% confluence and washed in Dulbecco's modified Eagle's medium without serum. Then they were incubated with 10 ng/mL recombinant human TNF-α (RnD Systems, Wiesbaden-Nordenstadt, Germany) and different PC species for various times at 37°C. Approximately 1 × 106 cells were collected in 300 μl lysis buffer from the MagnaPure mRNA Isolation Kit I (RAS, Mannheim, Germany) and mRNA was isolated with the MagnaPure-LC device using the mRNA-I standard protocol. RNA was reverse transcribed using AMV-RT and oligo- (dT) as the primer (First Strand cDNA synthesis kit, RAS), according to the manufacturer's protocol, in a thermocycler. Primer sets specific for the sequences of the selected genes optimised for the LightCycler (RAS) were developed and provided by SEARCH-LC GmbH, Heidelberg http://www.search-lc.com webcite. The PCR was performed with the LightCycler FastStart DNA Sybr GreenI kit (RAS) according to the protocol provided in the parameter specific kits. To control for the specificity of the amplification products, a melting curve analysis was performed. No amplification of unspecific products was observed. The copy number was calculated from a standard curve obtained by plotting known input concentrations of four different plasmids at log dilutions to the PCR cycle number at which the detected fluorescence intensity reaches a fixed value. This was done to reduce variations due to handling errors over several logarithmic dilution steps. To correct for differences in the content of mRNA, the calculated copy numbers were normalised according to the average expression of two housekeeping genes (Cyclophilin B and β-Actin). Values were thus given as input adjusted to the copy number per μl of cDNA.

Transient transfection and reporter assays

Caco-2 cells were seeded in 12-wells, grown to a >95% confluency and transiently transfected with a NF-κB-dependent luciferase reporter plasmid according to the manufacturer's instructions (Stratagene, La Jolla, USA). Cells were then co-treated in medium with or without TNF-α (10 ng/ml) and with a 200 μM solution of different PCs for 4 h at 37°C 20 h after transfection. In pre-treatment experiments, cells were first incubated for 10 minutes with 200 μmol PC, washed, and afterwards stimulated with TNF-α (10 ng/ml) only. Luciferase activity was assayed using the Luciferase Assay Kit (Stratagene) according to the manufacturer's directions and detected with a Fluorostar Optima (BMG Labtech, Offenburg, Germany). Each transfection was performed in triplicate and repeated at least three times.

Flow Cytometry

A 25 μl volume of washed cells (60% density, 2*105 cells), either pre-treated with a 200 μmol PC or left untreated, was incubated with 10 μl of biotinylated TNF-α (10 ng/mL) for 60 min at 4°C. Biotinylated soybean trypsin inhibitor was used as negative control. A 10 μl volume of avidin-FITC reagent was then added to each tube and incubated for an additional 30 min at 4°C in the dark. The cells were washed twice with 2 ml of 1× RDF1 buffer to remove unbound avidin-fluorescein and resuspended in 600 μl of 1× RDF1 buffer. The sample was then subjected to flow cytometric analysis by using 488 nm wavelength laser excitation (Beckman Coulter). As a test of specificity, TNF-α biotin was neutralized with an anti-TNF-α antibody and then added to the cells to block nonspecific and specific binding of TNF-α biotin.

Preparation of DRMs

Detergent extraction with Triton X-100 was performed as described [22]. Cells were grown in 3.5 cm dishes, transfected with TNF-α-R1 and TNF-α-R2 (provided by J. R. Turner, University of Chicago) and 10–12 h later washed once with PBS and scraped on ice into 1.5 ml homogenisation buffer (250 mM Sucrose, 10 mM Hepes, 2 mM EDTA). After centrifugation (5 min at 2000 rpm), cell pellets were homogenised in a homogenisation buffer containing 20 μg/ml each of chymostatin, leupeptin, antipain and pepstatin A (Sigma) through a 26 G needle and centrifuged for 5 min at 3000 rpm. The resulting supernatant was subjected to extraction for 30 min at 4°C in 1% Triton X-100. The extracts were adjusted to 40% OptiPrep (Axis-Shield, Oslo, Norway) and overlaid in a TLS 55 centrifugation tube with 30% OptiPrep/TNE and TNE (25 mM Tris-HCl, pH 7.4, 150 mM NaCl, 2 mM EDTA old protocol/25 mM Tris-HCl, pH 10.8, 150 mM NaCl, 5 mM EDTA). The gradients were centrifuged at 400000 g in a Beckman SW41 rotor for 20 h at 4°C. Fractions were obtained and used for Western blotting as described [23]. Monoclonal antibodies against TNF-α receptor 1 (TNF-α-R1) were from Sigma and TNF-α receptor 2 (TNF-α-R2) from Alexis Biochemical (Lörrach, Germany); monoclonal antibodies against the Src-like kinase Yes were supplied from Transduction Laboratories (Lexington, K Y); and against Flotillin-1 came from BD Bioscience (Heidelberg, Germany).

Statistical analysis

All values are reported as mean and standard deviation (SD) or standard error of the mean (SEM). For homogeneity of variance, ANOVA was applied. Significance levels between single groups (medium, +TNF-α, +TNF-α +phospholipid) were analysed using Tukey's post-hoc test. Probability values of p < 0.05 were set as a threshold for statistical significance.

Results

Different species of PC inhibit TNF-α-induced NF-κB activation in Caco-2 cells

Within our study, we tested the effect of several PC species (LPC 16:0, PC 18:2/18:2, PC 16:0/16:0, and PC 16:0/18:2) on the TNF-α-induced p65 promoter binding. First, Caco-2 cells were co-treated with TNF-α (10 ng) and PC. The promoter binding of p65 was detected by transient expression of a NF-κB luciferase reporter system and compared to the state of untreated cells. All PC species tested significantly inhibited the activation of NF-κB. As more unsaturated fatty acids the PC molecule had as more effective was the compound. The strongest effects were seen with LPC 16:0 (1-palmitoyl-glycero-3-PC) followed by PC 18:2/18:2 (1, 2-dilinoleoyl-glycero-3-PC). PC 16:0/16:0 was least effective. The effect was dose dependent for all PC species as previously shown for PC 18:2/18:2 [11] (see Additional file 1).

Additional file 1. Co-treatment of Caco-2 cells with TNF-α and phospholipids. Cells were grown in 3.5 cm dishes and the effects of different PC species on the inhibition of TNF-α-induced NF-κB-activation were analysed via the transient expression of a NF-κB-luciferase reporter system. (A) Cells were co-treated with 10 ng TNF-α and 200 μmol of the respective lipid. Luciferase activity was analysed 4 h after stimulation. Interestingly, PC 18:2/18:2 (1, 2-dilinoleoyl-glycero-3-PC), a PC species with two unsaturated side chains, was the most effective one compared to both PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) and PC 16:0/18:2 (1-palmitoyl-2-linoleoyl-glycero-3-PC) (p < 0.05). (B) Cells were co-treated with 10 ng/ml TNF-α and the indicated amounts of PC 16:0/16:0. PC inhibited NF-κB activation in a dose-dependent manner. The strongest effect was seen with 200 μmol PC which was significantly different from all other PC concentrations tested. The value was arbitrarily set to 100% in cells treated with TNF-α but not with phospholipids. Results presented here are representative for three others carried out independently. Data are shown as mean and SD (n = 3). Asterisks assign statistically different values from Tukey's post hoc test compared to control (*p < 0.05; **p < 0.01; ***p < 0.001); crosses indicate significant differences from +TNF-α after treatment with different phospholipids or phospholipid concentrations (+ p < 0.05; ++ p < 0.01; +++ p < 0.001).

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Whenever a co-treatment experiment is performed, there is a risk that the applied substances could interfere with each other within the medium. Therefore, we also tested whether the pre-incubation of our cells with PC (pre-treatment) is effective. Cells were first incubated with the respective lipid, washed and subsequently stimulated with TNF-α. Interestingly, pre-treatment resulted in a time-dependent inhibition of the NF-κB activation. Within the first 30 min, NF-κB activation decreased with increasing time of pre-treatment. Pre-treatment for longer time periods did not show any additional effect (p > 0.05) (Figure 1). [3H]-PC uptake kinetics revealed that the internalisation of PC was almost linear within the first 5 min and thereafter reached a plateau that possible explains why no additional effect on NF-kB activation was seen with longer pre-treatment times (see Additional file 2[24]).

Additional file 2. Uptake of [3H]-PC 16:0/16:0 into Caco-2 cells. To investigate whether the time-dependent inhibition of NF-κB activation correlates to the amount of PC taken up into the cells, we analysed the uptake of [3H]-PC 16:0/16:0. Methods: Caco-2 cells were grown to 80% confluence in 5 cm2 dishes and incubated for various times with different concentrations of 1-, 2-dipalmitoyl-3-phosphatidyl-[N-methyl-[3H]-choline ([3H]-PC, 81 Ci/mM) and 1-, 2-dipalmitoyl-glycero-3-phosphocholine (PC 16:0/16:0) at a ratio of 1:250. After washing, cells were incubated with NaOH (1 M) for 10 min. Both the cell lysates and the supernatants were analysed with counting solution in a scintillation counter (Beckman Coulter LS 6500) as done previously [11,24]. [3H]-methyl-choline]-L-dipalmitoyl-phosphatidylcholine ([3H]-PC) (50 Ci/mmol) was purchased from New England Nulcear, (Boston, MA, USA). Results: (A) The uptake reaches a plateau with increasing time. (B) Within the first 5 min of incubation with PC, the uptake was almost linear. An additional PC uptake was not detectable after 1 h. This uptake kinetic probably indicates that the inhibitory effect of exogenous PC correlates to the amount of PC incorporated into the cells. The plateau after 1 h likely explains why no additional effect on NF-κB activation was seen with longer pre-treatment times (Figure 1). Data are expressed as mean and SD of n = 5 experiments.

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thumbnailFigure 1. Pre-incubation with a 200 μM solution of PC resulted in a time-dependent inhibition of TNF-α induced NF-κB activation. NF-κB-activation was analysed via the transient expression of a NF-κB luciferase reporter system in Caco-2 cells. Cells were pre-treated with PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) for 5–120 min, washed and exposed for 4 h to 10 ng/ml TNF-α. The value was arbitrarily set to 100% in cells treated with TNF-α but not with lipid pre-treatment. Results presented here are representative for three others carried out independently. Data are expressed as mean and SD (n = 3). Asterisks assign statistically different values from Tukey's post hoc test compared to +TNF-α (*p < 0.05; **p < 0.01; ***p < 0.001).

Expression of pro-inflammatory genes is attenuated by PC

In previous publications, we have already shown that PC has an effect on pro-inflammatory gene transcription downstream of NF-κB [11]. In order to evaluate this effect in more detail, we analysed longer time periods and an extended set of genes. Caco-2 cells were stimulated with 10 ng/mL TNF-α for various times (30 to 240 min). Thereafter, mRNA was isolated to analyse the transcriptional levels by quantitative RT-PCR. Using this method, a significant up-regulation of IL-8, ICAM-1, IP-10, MCP-1, TNF-α and MMP-1 could be detected compared to the mRNA level of untreated cells (control) (p < 0.05) (see Additional file 3). Other genes (Cox-2, IL-10, IL-18, 4-1BB, ENA-78, TGFβ1) failed to be up-regulated by TNF-α (p > 0.05). After co-treatment of cells with PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) (+TNF-α +PC), the TNF-α effect was significantly reduced (p < 0.05). Similar effects were found for the treatment with LPC 16:0 (1-palmitoyl-glycero-3-PC). For evaluation of substrate specificity, we also tested the effect of PE 16:1/16:1 (1,2-dioleyl-glycerol-3-phosphatidylethanolamine (PE)). Co-treatment of cells with TNF-α and PE did not show any significant effect on the transcriptional level of ICAM-1, IP-10, MCP-1, TNF-α, MMP-1, Cox-2, IL-10, IL-18, 4-1BB, ENA-78 or TGFβ1 compared to TNF-α alone (p > 0.05).

Additional file 3. Effect of PC 16:0/16:0 on up-regulation of selected pro-inflammatory genes after TNF-α stimulation. Sub-confluent Caco-2 cells were stimulated with 10 ng/ml TNF-α to induce an up-regulation of MMP-1, IL-8, ICAM-1, MCP-1 and IP-10, which are known to be pro-inflammatory. (A) Co-treatment with 200 μmol of PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) resulted in a significant inhibition of the TNF-α-induced up-regulation. Up-regulation of selected genes after TNF-α stimulation might be classified into two groups: 1) early up-regulated genes (such as IL-8) and 2) late genes (ICAM-1, IP-10, MCP-1). The experiment depicted is representative of three others with the same results. Data are expressed as mean and SEM (n = 3). Asterisks assign statistically different values from Tukey's post hoc test (*p < 0.05; **p < 0.01; ***p < 0.001) comparing +TNF-α and +TNF-α +PC at each time point; crosses indicate significant differences of control compared to both +TNF-α and +TNF-α +PC at each time point (+ p < 0.05; ++ p < 0.01; +++ p < 0.001).

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Interestingly, some genes were up-regulated faster than others. This led us to classify the genes into two groups: 1) early up-regulated genes (IL-8, TNF-α), where a significant increase in transcript levels could be detected within 30 min; and 2) late up-regulated genes (ICAM-1, MCP-1, IP10, MMP-1) which responded later. PC pre-treatment reduced the transcriptional levels of both groups of genes significantly. The effect lasted for up to 120 min. Analysing later time points (240 min) did not show a significant difference anymore. The only exception was MMP-1, where a significant difference could also be detected after 240 min (see Additional file 3). This observation may be due to metabolic effects.

The effect of PC on the expression levels of selected genes is comparable to the effect of the NF-κB inhibitor SN 50

It is known that the cytokine-induced expression of IL-8, MCP-1, COX-2 and other genes involved in inflammation is highly dependent on the transcription factor NF-κB [25-27]. An inhibitory effect of PC on the activation of the MAPkinases ERK and p38 have been previously described [11]. If we extend this by hypothesizing that PC inhibits TNF-α induced NF-κB activation and the subsequent pro-inflammatory gene transcription upstream of NF-κB, we could expect similar effects on gene transcription by inhibiting NF-κB in a direct way. Therefore we carried out experiments with the specific NF-κB-inhibitor SN 50. Pre-incubation of Caco-2 cells with SN 50 for 30 min before stimulation with TNF-α (10 ng/mL) resulted in a significantly reduced up-regulation of IL-8, ICAM-1, MCP-1 and IP-10. The inhibitory effects with SN 50 were as strong as the effects seen after pre-incubation with 200 μmol of either PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) (see Additional file 4) or LPC 16:0 (1-palmitoyl-glycero-3-PC) (data not shown). Therefore, the inhibitory effect of PC seems to be regulated within the TNF-α/NF-κB-pathway probably upstream of NF-κB.

Additional file 4. Effect of SN 50 and PC on TNF-α-induced gene activation. Sub-confluent Caco-2 cells were stimulated with TNF-α (10 ng/mL) to induce an up-regulation of several selected genes. Pre-treatment with the NF-κB inhibitor SN 50 (50 mg/mL) for 30 min resulted in a significant reduction of the TNF-α-induced up-regulation. This reduction was similar to that found in cells treated with PC, possibly indicating that both treatments influence the same pathway. Data are expressed as mean and SEM (n = 3). Asterisks assign statistically different values from Tukey's post hoc test of +TNF-α to all other values at each time point (*p < 0.05; **p < 0.01; ***p < 0.001); At no time point could a significant difference of +TNF-α +PC and +TNF-α +SN 50 be detected with the exception ICAM-1 at 120 min. Crosses indicate significant differences of control compared to +TNF-α, TNF-α +SN 50 and +TNF-α +PC at each time point (+ p < 0.05; ++ p < 0.01; +++ p < 0.001).

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PC has no effect on the binding of TNF-α to its receptors

To exclude the possibility that PC might be acting by inhibiting the interaction of TNF-α to its receptors, we performed FACS analyses using biotin labeled TNF-α and avidin-FITC. The interaction of TNF-α with its receptor was readily and reproducibly observed in cells treated with either TNF-α-biotin alone or with cells pre-incubated for 1 h prior to the addition of TNF-α-biotin with 200 μmol of either PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) or PC 18:2/18:2 (1, 2-dilinoleoyl-glycero-3-PC). None of the tested PC species affected the interaction of TNF-α to its receptors or changed the density of TNF-α receptors at the cell surface (see Additional file 5).

Additional file 5. Neither PC 16:0/16:0 nor PC 18:2/18:2 showed any effect on the binding of TNF-α to its cell surface receptors. Vero cells were taken for FACS analyses because of their regular cell shape. They were either left untreated or were pre-treated for 1 h prior to the addition of TNF-α-biotin with a 200 μM preparation of PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) or PC 18:2/18:2 (1, 2-dilinoleoyl-glycero-3-PC). The PC-treated (TNF-α-biotin + PC 16:0/16:0 or TNF-α-biotin + PC 18:2/18:2) and untreated (TNF-α-biotin) cells were then collected for staining with biotinylated TNF-α and avidin-FITC. Soybean trypsin inhibitor that had been biotinylated in the same degree was used as a negative control. Neutralized TNF-α biotin with anti-TNF-α blocking antibody was used as a specificity control. Receptor binding activity was determined by flow cytometric analysis with a 488 nm wavelength laser excitation. Results shown here were representative for three other experiments carried out independently.

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PC and LPC changes compartmentation of TNF-α-R1 and TNF-α-R2 to lipid rafts at the plasma membrane

We have previously shown that PC can inhibit the TNF-α-induced activation of the MAPkinases ERK and p38 [11]. If the effect of PC on TNF-α-induced gene transcription were indeed to take place upstream of NF-κB activation, it would possibly happen because of the lipophilic character of the substance within or at the plasma membrane. It has been previously shown that TNF-α receptors reside at the plasma membrane at least partially in lipid rafts and it has been suggested that compartmentation influences the signalling response [28]. As shown in Figure 2, PC does not change the concentration of TNF-α receptors at the cell surface. Therefore, we hypothesized that PC might not change the overall concentration but possibly the compartmentation of TNF-α receptors within the plasma membrane. DRMs were prepared in order to evaluate this hypothesis. Caco-2 cells were transfected with TNF-α-R1 and TNF-α-R2 and then extracted with Triton X-100 and subjected to OptiPrep step gradient centrifugation. TNF-α-R1 and TNF-α-R2 were found in two pools in cellular membranes, one within the DRMs and one outside of the DRMs. PC or LPC treatment shifted both receptors towards an increased DRM association (Figure 2). PC and LPC induced also an increased DRM association for the raft marker proteins Yes and Flotillin-1 (data not shown) that served as controls.

thumbnailFigure 2. This figure represents the effect of both LPC and PC on the association of TNF-α-R1 and TNF-α-R2 to DRMs. COS cells were lysed in 1% Triton X-100 at 4°C 20 h after transient transfection of TNF-α-R1 and TNF-α-R2. After floatation in an OptiPrep step-gradient, TNF-α-R1 and TNF-α-R2 were found in two pools, in DRMs (lane 7–8) and in soluble membranes (lane 1–4). Pre-treatment with 200 μmol LPC or PC resulted in an increased DRM association.

PC inhibits the TNF-α-induced up-regulation of selected genes from the apical and basolateral sides of fully polarised Caco-2 cells

Based on the results with non-polarised cells, we also carried out analyses with fully polarised, filter grown Caco-2 cells. To establish this system, we tried out several conditions to stimulate the cells. It has been previously described that in fully polarised Caco-2 cells, the TNF-α-receptor is localised at the basolateral side and therefore not accessible for TNF-α applied to the apical surface [29,30]. We could confirm this finding by analysing the transcriptional level of selected genes after stimulating the cells with TNF-α from the apical and basolateral sides. An up-regulation could only be detected after stimulation from the basolateral side (Figure 3). Interestingly, PC and LPC inhibited TNF-α-induced gene transcription from both domains (Figure 4).

thumbnailFigure 3. This figure shows the effect of TNF-α from the apical and basal sides on gene transcription. Caco-2 cells were grown in a 6-transwell system and stimulated with TNF-α (50 ng/mL) to induce an up-regulation of several selected genes involved in inflammation. Only basolateral stimulation with TNF-α (TNF-α bl) resulted in a significant up-regulation while apical stimulation with TNF-α (TNF-α ap) did not show any significant effect (p > 0.05). Data are expressed as mean and SD of n = 3 experiments. Asterisks assign statistically different values comparing apical and basolateral stimulation (*p < 0.05; **p < 0.01; ***p < 0.001).

thumbnailFigure 4. PC inhibits pro-inflammatory gene transcription from both the apical and basolateral sides of polarised Caco-2 cells. Polarised Caco-2 cells were grown in a 12-transwell system and stimulated with TNF-α (50 ng/mL) from the basolateral side to induce an up-regulation of several genes (IL-8, IP-10, and MMP-1) involved in inflammation (TNF-α). Both basolateral (+TNF-α +PC bl) and apical (+TNF-α +PC ap) treatments with 200 μmol of PC 16:0/16:0 (1, 2-dipalmitoyl-glycero-3-PC) resulted in a significant reduction in the TNF-α-induced up-regulation. Asterisks assign statistically different values from Tukey's post hoc test of TNF-α to all other values at each time point (*p < 0.05; **p < 0.01; ***p < 0.001); At no time point could a significant difference of +TNF-α +PC ap and +TNF-α +PC bl be detected; crosses indicate significant differences of control compared to both +TNF-α and +TNFα +PC at each time point (+ p < 0.05; ++ p < 0.01; +++ p < 0.001).

Discussion

The data we have presented here further strengthens the evidence that the application of exogenous PC has anti-inflammatory effects. Firstly, we could confirm that different PC species can inhibit TNF-α-induced NF-κB activation. LPC functioned in the same way, whereas PE was not effective. The effect of PC was not merely transient but instead persisted for at least for 2 h. Consistent with previous results [11], we could demonstrate that the effect is dose dependent. Interestingly, PC 16:0/16:0 was less effective than species with unsaturated fatty acid side chains. As human mucus is made up of more than 90% PC species with one unsaturated fatty acid side chain (PC 16:0/18:1; PC 16:0/18:2; PC 18:0/18:1 and PC 18:0/18:2) [5], it is intriguing to speculate that this might represent an optimal mixture for controlling the inflammatory response. The hypothesis deduced from this is that mucus PC might be a source for membrane PC in enterocytes and thus influence membrane-dependent signalling of the mucosa cells.

Clinical and animal as well as in vitro data further support the anti-inflammatory effect of PC. We and others have previously shown that PC inhibits actin polymerisation on isolated phagosomes as well as in macrophages and Caco-2 cells [11,12]. In the latter model, it also inhibits activation of the MAPkinases ERK and p38, which are upstream of NF-κB [11]. Many animal studies support that PC is protective against pro-inflammatory conditions. With respect to this, it as been shown that it prevents mucosal injury induced by acids, NSAIDs or bile acids [9,31-39]. Parenteral administration of PC or LPC has been demonstrated to increase survival and improve inflammation in animal models of acute septic shock and endotoxemia [40-42]. Interestingly, there is a sudden overproduction of TNF-α in acute septic shock which triggers hypotension, circulatory collapse, and the widespread inflammation seen in this clinical condition [43]. Various species of LPC seem to protect against such a condition [42]. TNF-α is also thought to be an important agent in the colonic inflammation of patients with ulcerative colitis (UC). There is an increased density of TNF-α immunoreactive cells in the mucosa of UC patients with actual inflammation and there is an increased concentration of TNF-α in faeces, mucosa biopsies and serum of actively ill patients [44-46]. Most importantly, clinical studies have revealed that an anti-TNF-α strategy can be successful in treating those patients; therefore, this strategy is now integrated in daily clinical practice [47]. Two clinical studies on patients with ulcerative colitis have been performed which show a therapeutic benefit by adding PC in the form of slow release preparations [6,7]. In these studies, PC was applied in the form of soy lecithin with a considerable amount of PE. PE can be metabolised to PC via methylation and therefore serves as an additional source for PC within the cell. PE is also a known source for the endocannabinoid system, which influences inflammatory reactions as well [48]. However, our data show that exogenous PE has no significant effect on TNF-α-induced activation. This probably means that it is not the effective component of the preparation used in the clinical trials.

TNF-α exerts its functions through two distinct receptors, TNF-α-R1 (CD120a) and TNF-α-R2 (CD120b). After binding TNF-α, TNF-α-R1 recruits a death domain (DD)-containing adaptor molecule, namely the TNF-α-R1-associated death domain protein (TRADD). TRADD serves as a platform for recruiting additional mediators [49]. It binds the DD-containing Ser/Thr kinase receptor-interacting protein (RIP) and TNF-receptor-associated factor 2 (TRAF2). This TRADD-RIP-TRAF2 complex initiates the pathway leading to NF-kB activation [50-52]. How might exogenous PC function in this regulation?

1. It could be speculated that PC or LPC inhibits the association of TNF-α to its receptor. To exclude such an effect, we performed experiments in which the cells were treated with PC before TNF-α stimulation and quantified the binding of TNF-α to its receptor by FACS. FACS analysis could detect no quantitative differences between PC or LPC treated and non-treated cells. This makes a decreased receptor binding unlikely.

2. It has been previously suggested that TNF-α receptors, upon substrate binding, might be endocytosed and that the signalling response occurs in endosomes, as demonstrated in other receptors such as the β2-adrenergic receptor, the endothelin receptor and many other G-coupled protein receptors [53-56]. Thus it has been speculated that the integration of PC into cellular membranes might affect endocytosis and consequently signalling. However, we could show by FACS analysis that the surface expression of TNF-α receptors was unchanged after PC treatment. This makes an influence of PC on endocytosis also unlikely.

3. A third scenario seems more likely. Mammalian membranes are lipid bilayers consisting of 300–400 different lipid species that are ordered in vertical and lateral dimensions. This order is maintained with the help of a highly regulated concert of enzymes. Adding exogenous lipids would lead to a change in the lipid assembly of the membrane and therefore would influence membrane-dependent processes. We have previously speculated that PC might be present in a freely mobile form and a pool that is attached to proteins [11]. Proteins that bind selectively to PC have been described (e.g., START, C1 or C2 domain structures), of which a large number are involved in signalling [57,58]. Adding PC might shift the balance between the free and the bound fractions. Normally in cells the bulk of PC is in the outer leaflet of the membrane. It is therefore also possible that addition of PC might induce a higher concentration of PC on the inner leaflet. There it could interfere with selected signalling proteins such as MAP kinases or others involved in NF-κB activation. However, it has to be mentioned that the role of NF-κB is more complex in regulating the answer of the intestinal epithelium to luminal agents. NF-κB has been shown to regulate protective factors as well, including inducible beta defensins [59]. Epithelial-cell-specific inhibition of NF-kB through conditional ablation of NEMO (IKKgamma) led to an increased apoptosis of colonocytes, impaired expression of antimicrobial peptides and translocation of bacteria into the mucosa [60]. NF-κB therefore seems to be a regulator for the intestinal immune homoeostasis and the tuning of its activity by many mechanisms appears crucial in preventing inflammation [61]. The pool of membrane PC could be a part of this regulation.

4. Not only proteins but also membrane lipid compartments are necessary for TNF-α signalling to occur. It has been previously shown that TNF-α binding recruits TNF-α-R1 to lipid rafts [28]. Rafts are small platforms composed of sphingolipids and cholesterol in the outer exoplasmic leaflet and connected to phospholipids and cholesterol in the inner cytoplasmic leaflet of the lipid bilayer [62]. These assemblies are fluid but more ordered and tightly packed than the surrounding bilayer. The difference in packing is due to the saturation of the hydrocarbon chains in raft sphingolipids and phospholipids as compared with the unsaturated state of fatty acids of phospholipids in the surrounding bilayer [62]. Therefore it is possible that a change in the phospholipid concentration within the membrane has an impact on the lipid raft integrity. Discrepancies in the localisation of TNF-α-R1 to lipid rafts exist. Although in U937 and NIH-3T3 cells TNF-α-Rs were found mainly in lipid rafts and were shifted to detergent soluble parts upon TNF-α stimulation [63], TNF-α increased their lipid raft association in HeLa [64] and HT1080 fibrosarcoma cells [65]. Conflicting data also exist concerning a compartmentalised NF-kB activation. Whereas some authors claim that NF-kB activation by TNF-α occurs in lipid raft domains [28] other publications suggest a lipid-raft-independent activation [63]. However, our data showed that upon exposure of Caco-2 cells with PC or LPC, the lipid raft associations of both TNF-α-R1 and TNF-α-R2 are increased and both lipids were inhibitory in our setting. Therefore, we assume that TNF-α-induced NF-kB activation occurs outside lipid rafts.

To get closer to the scenario in the mucosa, polarised Caco-2 cells were analysed as well. Although polarised cells could only be stimulated by basolateral exposure to TNF-α, an inhibitory effect of PC could be observed from both the apical and basolateral sides. The cause of this phenomenon requires further investigation; however, a possible explanation may be that TNF-α signalling occurs after internalisation and that apical and basolateral vesicles mix with each other in the endosomal compartments [56]. Another possible explanation is that PC is integrated and rapidly exchanged between the apical and basolateral domains via the inner layer of the plasma membrane [66].

Conclusion

In summary, our results further support the idea that exogenous PC and LPC have anti-inflammatory properties. Our findings suggest that PC (LPC) inhibits the signalling responses via NF-κB possibly due to changes in the plasma membrane. This is a potential mechanism explaining how PC can influence the course of ulcerative colitis and provides the molecular foundation for the benefit seen in our clinical studies.

Abbreviations

DD: death domain; DRMs: detergent resistant membranes; IBD: inflammatory bowel disease; ICAM-1: intercellular adhesion molecule 1; IL-8, -1β: interleukin 8, 1β; IP-10: interferon inducible protein 10; LPC: lysophosphatidylcholine; MCP-1, -2, and -3: monocyte chemoattractant proteins 1, 2, and 3; NF-κB: nuclear factor-κB; ns: not significant; PC: phosphatidylcholine; PE: phosphatidylethanolamine; RIP: receptor-interacting protein; SD: standard deviation; SEM: standard error of the mean; SM: sphingomyelin; TNF-α: tumour necrosis factor α; TNF-α-R21, -R2: tumour necrosis factor α receptor 1, receptor 2; TRADD: TNF-α-R1-associated death domain protein; TRAF2: TNF-receptor-associated factor 2; UC: ulcerative colitis.

Competing interests

The authors declare that they have no competing interests.

Authors' contributions

RE precipitated in the design of the study and in the data analysis. He drafted the manuscript. AB, IT and PJ carried out the experiments. TG performed the RT-PCR analysis. JF, WS and GG were involved in the design of the study. All authors read and approved the final manuscript.

Acknowledgements

IT was financed by the Y.I.A. of the Medical Faculty of Heidelberg. JF and RE were supported by a grant of the Stiftung Nephrologie. JF, RE and WS were supported by the Hopp Foundation.

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Pre-publication history

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