Departments of 1Critical Care Medicine, 3Pathology, and 2Surgery, University of Pittsburgh School of Medicine, Pittsburgh, Pennsylvania 15261
Submitted 13 June 2003 ; accepted in final form 28 July 2003
![]() |
ABSTRACT |
---|
![]() ![]() ![]() ![]() ![]() ![]() |
---|
zonula occludens-1; occludin; nitric oxide; permeability; multiple organ dysfunction syndrome; inducible nitric oxide synthase; lipopolysaccharide
The normal functioning of the lung depends on the establishment and maintenance of a milieu in the alveolar space that is distinct from the composition of the subepithelial compartment. This process depends on the formation and proper functioning of specialized structures, called tight junctions (TJ), between adjacent cells making up the epithelial sheet. The TJ is a complex of several integral membrane proteins and peripheral membrane proteins that interact strongly with the cytoskeleton (19). Integral membrane proteins involved in TJ formation include occludin and members of a large class of proteins called claudins (19). These proteins contain four transmembrane domains and are thought to be the points of cell-to-cell contact within the TJ (6). Cosedimentation assays of TJ proteins suggest that there is a strong interaction between occludin and another protein associated with TJ formation, zonula occludens (ZO)-1 (13, 36). ZO-1 has been shown to interact with the cytoplasmic tails of occludin and the claudins. In addition, ZO-1 interacts with two additional members of the membrane-associated guanylate kinase family of proteins, ZO-2 and ZO-3 (18). The TJ serves as a fence that differentiates the plasma membrane into apical and basolateral domains (51). TJs also serve as a regulated semipermeable barrier that limits the passive diffusion of solutes across the paracellular pathway between adjacent cells (2, 21). These properties of TJs, in combination with transcellular vectorial transport processes, generate distinct internal environments in the opposing compartments.
Nitric oxide (NO), a simple diatomic free radical, acts as a mediator of immune system function and cell signal transduction (26). Relatively large amounts of NO can be synthesized by the enzyme inducible NO synthase (iNOS). Induction of iNOS expression and increased NO biosynthesis on this basis have been identified in a variety of cell types in response to exposure to inflammatory cytokines and/or lipopolysaccharide (LPS; endotoxin) (29). Within the lung, a variety of cell types are capable of synthesizing and releasing NO, including macrophages, neutrophils, endothelial cells, vascular smooth muscle cells, and epithelial cells (5, 22, 29).
NO and other related reactive nitrogen species, notably peroxynitrite, are thought to play an important role in pathogenesis of pulmonary dysfunction associated with sepsis and other conditions associated with systemic inflammation (4, 23, 38, 45, 53). When cultured monolayers of various epithelial cell lines, including A549 pneumocyte-like (31) and Caco-2 enterocyte-like cells (10, 47), are stimulated with proinflammatory cytokines in vitro, barrier function is impaired. Increased levels of NO, whether generated endogenously after iNOS upregulation or derived from the spontaneous decomposition of an exogenous donor, interfere with the proper expression and targeting of several TJ proteins in cultured epithelial cells (8, 24, 52). Prompted by these findings, we hypothesized that increased production of NO might lead to structural and functional alterations in pulmonary TJ function in vivo as a result of a systemic inflammatory response induced by injecting mice with LPS. Herein, we show that endotoxemia is associated with decreased expression and function of several TJ proteins in the epithelium of lung.
![]() |
METHODS |
---|
![]() ![]() ![]() ![]() ![]() ![]() |
---|
Animals. This research complied with regulations regarding animal care as published by the National Institutes of Health and was approved by the Institutional Animal Use and Care Committee of the University of Pittsburgh. Male C57Bl/6J mice weighing 2025 g were from Jackson Laboratories (Bar Harbor, ME). All animals were maintained in the University of Pittsburgh Animal Research Facility on a 12-h light-dark cycle with free access to standard laboratory chow and water. Animals were not fasted before experiments. Animals were anesthetized before surgery by intramuscular injection with pentobarbital sodium (6090 mg/kg; Abbott Labs, Chicago, IL).
To induce a systemic inflammatory response, mice were injected intraperitoneally with Escherichia coli (strain O111:B4) LPS (50 µg/mouse; 2 mg/kg) dissolved in 1.0 ml of PBS. Control animals were injected with a similar volume of PBS without LPS. Some mice were treated with two 5-mg/kg doses of L-NIL administered by intraperitoneal injection 2 and 8 h after the injection of LPS or PBS. Some mice were treated with L-NIL according to the same schedule in the absence of a prior injection of LPS. Groups of mice were anesthetized 6, 12, or 18 h after injection of LPS or PBS for measuring lung epithelial barrier function or harvesting tissue specimens for various biochemical or histological assays.
Effect of cytomix on the permeability of Calu-3 monolayers. The Calu-3 cell line was obtained from American Type Culture Collection (no. HTB-55) and cultured on collagen I-coated Biocoat tissue culture dishes. Calu-3 cells are derived from a human lung adenocarcinoma and form epithelial monolayers when grown on permeable supports in culture (1). This cell line has been used to study lung epithelial permeability in vitro (1, 48). For permeability assays, 5 x 105 Calu-3 cells were seeded onto 24-well Transwell microporous inserts. Monolayers growing on Transwell inserts were used 14 days after seeding. The medium bathing the apical surface of the monolayers was replaced with 200 µl of DMEM complete medium (pH 6.8) containing FITC-dextran (average molecular mass 4,000 Da; FD4) at 25 mg/ml. The medium bathing the basolateral surface was replaced with 500 µl of DMEM complete medium alone or DMEM supplemented with cytomix (1,000 U/ml IFN-, 10 ng/ml TNF-
, and 1 ng/ml IL-1
) in the absence or presence of 100 µM L-NIL. The cells were then incubated for 6 or 12 h. The concentrations of FD4 in the apical and basolateral media were determined spectrofluorometrically with a Packard Fusion Reader (Packard Bioscience, Boston, MA) using an excitation filter of 492 nm and an emission wavelength of 515 nm. The permeability of the monolayers was expressed as a clearance (nl·cm-2·h-1) as described previously (24).
Measurement of bronchoalveolar epithelial permeability. Mice were injected via the tail vein with either FD4 solution in PBS (25 mg/ml; 10 mg/kg) or FITC-labeled bovine serum albumin (FITC-albumin; 1.25 mg/ml; 5 mg/kg). Ten minutes later for mice injected with FD4 or 2 h later for mice injected with FITC-albumin, the animals were anesthetized. The trachea was exposed, and the lungs were lavaged three times with 1 ml of sterile saline per wash. The aliquots of bronchoalveolar lavage fluid (BALF) were pooled, and fluorescence was determined as described above. Blood was obtained by cardiac puncture, and the serum was collected. Ten microliters of serum were mixed with 200 µl of PBS, and fluorescence was determined as described above. The BALF:serum fluorescence ratio was calculated and used as a measure of pulmonary epithelial permeability.
Measurement of NO production. Aliquots of BALF and serum were cleared by centrifugation. The end products of NO metabolism, , were quantitated using the Bioxytech Nitric Oxide Assay kit exactly as directed by the manufacturer (OXIS International, Portland, OR).
Nonidet P-40-insoluble and total protein extracts. Lung tissue (150200 mg) was homogenized on ice with a Polytron tissue homogenizer in 1 ml of Nonidet P-40 (NP-40) lysis buffer [25 mM HEPES, pH 7.4, 150 mM NaCl, 4 mM EDTA, 25 mM NaF, 1% NP-40, 1 mM Na3VO4, 1 mM 4-amidinophenylmethanesulfonyl fluoride (APMSF), 10 µg/ml leupeptin, and 10 µg/ml aprotinin]. The samples were gently rocked at 4°C for 30 min. The sample was centrifuged at 12,000 g for 30 min at 4°C. The pellets were resuspended in SDS-dissolving buffer (25 mM HEPES, pH 7.5, 4 mM EDTA, 25 mM NaF, 1% SDS, and 1 mM Na3VO4) using five strokes with a Dounce homogenizer (pestle B) followed by sonication with a 0.1 W Fisher Scientific Sonic Dismembrator fitted with a microtip on power setting three. Sonication continued until the precipitate was completely dissolved. These were designated the NP-40-insoluble fractions.
For total cellular protein extracts, tissue specimens were homogenized in cold RIPA buffer [PBS, 1% NP-40, 0.5% sodium deoxycholate, 0.1% SDS, 0.1 mg/ml APMSF, 1.0 mM sodium orthovanadate, and 1x mammalian protease inhibitor cocktail (Sigma-Aldrich cat. no. P 8340)] and sonicated until the sample was completely dissolved. These samples are referred to as total protein extracts.
Immunoprecipitation. One hundred micrograms of NP-40-insoluble fraction were immunoprecipitated with either anti-occludin or anti-ZO-1 polyclonal antibodies. The lysate was precleared by adding 0.25 µg of normal mouse IgG together with 20 µl of suspended protein A/G agarose (Santa Cruz Biotechnology, Santa Cruz, CA). After being incubated at 4°C for 30 min, the beads were collected by centrifugation at 2,500 rpm for 5 min at 4°C. The supernatant was transferred to a fresh tube, 3 µg of anti-occludin or anti-ZO-1 antibody were added, and the tube was incubated on a rocker platform for 2 h at 4°C. Twenty microliters of resuspended agarose A/G were added to the tube, and the incubation was continued overnight at 4°C with gentle shaking. The agarose beads were washed five times with 1 ml of NP-40 lysis buffer. Proteins were eluted by boiling in 1x Laemmli buffer (10% glycerol, 5% 2-mercaptoethanol, 2.5% SDS, 0.1 M Tris, pH 6.8, and 0.2% bromphenol blue) for 10 min. Equal volumes of sample were separated by gel electrophoresis followed by immunoblotting.
Immunoblotting. Equal amounts of total protein extract were mixed in 1x Laemmli buffer, boiled for 3 min, and centrifuged for 10 s. The supernatants were electrophoresed on 7.5% or 12% precast SDS-polyacrylamide gels (Bio-Rad, Hercules, CA). The proteins were electroblotted onto Hybond-P polyvinylidene difluoride membranes (Amersham Pharmacia Biotech, Leicester, UK) and blocked with Blotto (1x Tris-buffered saline, 5% milk, 0.05% Tween 20, and 0.2% NaN3) or 1:10 normal donkey serum (ZO-2 and ZO-3 only) for 60 min. The filters were incubated at room temperature for 1 h with anti-ZO-1 or anti--actin antibody at a 1:4,000 dilution or anti-ZO-2, anti-ZO-3, or anti-iNOS antibody diluted 1:2,000 in PBST (PBS and 0.02% Tween 20). After being washed three times in PBST, immunoblots were exposed for 1 h to a 1:20,000 dilution of the appropriate horseradish peroxidase-conjugated secondary antibody. After three washes in PBST and two washes in PBS, the membrane was impregnated with an enhanced chemiluminescence substrate (ECL, Amersham Pharmacia Biotech) and used to expose X-ray film. Autoradiographs were captured using a Hewlett Packard (Palo Alto, CA) ScanJet 6300s. Band intensities were quantified by densitometry and expressed as mean area density using GelExpert 3.5 software (Nucleotech, San Mateo, CA). For total protein blots, mean area density is expressed relative to
-actin expression.
Immunofluorescence. Frozen tissue sections (8 µm) were prefixed in cold acetone and then air-dried. The sections were fixed with 4% paraformaldehyde and then washed three times with cold PBS. The sections were blocked with 10% donkey serum. Tissue sections were incubated with primary antibodies as follows: rabbit anti-ZO-1 polyclonal antibody and rabbit anti-occludin polyclonal antibody. Some sections were incubated with PBS alone in place of a primary antibody as a negative control. After a 1-h incubation at room temperature, the sections were washed three times with PBS. Tetramethylrhodamine isothiocyanate-conjugated goat anti-rabbit secondary antibody was added and incubated for 45 min at room temperature. The sections were washed three times with PBS, and the nuclei were stained with 4',6-diamidino-2-phenylindole dihydrochloride (Molecular Probes, Eugene, OR). Coverslips were mounted using the Molecular Probes Antifade kit. Thin sections were obtained from paraffin-embedded tissue specimens and stained with hematoxylin and eosin. Images were captured using an Olympus Provis fluorescence microscope.
Assessment of NF-B activation. Briefly, we homogenized murine tissue samples with tissue protein extraction reagent (Pierce, Rockford, IL). The EMSA for NF-
B nuclear binding was performed using a radiolabeled duplex oligonucleotide obtained from Promega (Madison, WI). The detailed methods for the EMSA have been described previously (50).
Statistical analyses. Results are presented as means ± SE. Data were analyzed using analysis of variance followed by Fisher's least significant differences test. P values <0.05 were considered significant.
![]() |
RESULTS |
---|
![]() ![]() ![]() ![]() ![]() ![]() |
---|
|
We extended these observations by examining the effect of E. coli LPS (2 mg/kg) on the leakage of FD4 or FITC-albumin from the plasma compartment into the alveolar space in C57Bl/6J mice. At various time points after injection of LPS or PBS, we injected mice with FD4 in saline. Within 6 h after the induction of endotoxemia, the BALF:serum FD4 ratio increased significantly (Fig. 2A). At 12 h, the BALF:serum FD4 ratio increased still further. By 18 h after the injection of LPS, the BALF:serum FD4 ratio had returned toward normal. Delayed treatment with L-NIL significantly ameliorated the increase in lung permeability caused by LPS. When we used FITC-albumin instead of FD4 as permeability probe, we observed similar changes, although the magnitude of the effect was much smaller, and the results were less reproducible. Twelve hours after the injection of LPS, the BALF:serum FITC-albumin ratio increased but the change was not statistically significant. Treatment of mice with L-NIL ameliorated the slight increase in lung-to-BALF leakage of FITC-albumin induced by injection of LPS (Fig. 2B). We interpret these findings as indicating that the BALF:serum FD4 ratio is more sensitive than the BALF:serum FITC-albumin ratio for detecting changes in bronchoalveolar epithelial permeability, presumably because leakage of the larger probe is probably also influenced by the integrity of the alveolar endothelial barrier. We also interpret these findings as showing that injecting mice with LPS transiently impairs bronchoalveolar epithelial barrier function. Finally, these data support the view that LPS-induced bronchoalveolar barrier dysfunction is mediated, at least in part, by iNOS-dependent NO synthesis.
|
Injecting mice with LPS significantly increased the concentration of the NO breakdown products and
in BALF (Fig. 3A) and serum (Fig. 3B). Treatment with L-NIL only partially inhibited the accumulation of
and
in blood, whereas treatment with the iNOS inhibitor almost completely blocked accumulation of these NO metabolites in BALF.
|
Endotoxemia is associated with NF-B activation in lung tissue and increased pulmonary iNOS expression. Induction of iNOS expression in macrophages (27) and pulmonary epithelial cells (38) is at least partially controlled by the transcription factor NF-
B. As expected, we documented LPS-induced NF-
B activation and upregulation of iNOS expression using EMSA (Fig. 4A) and Western blotting (Fig. 4B) in lung tissue extracts, respectively.
|
Endotoxemia is associated with alterations in the expression of TJ proteins in the lung. NP-40-insoluble occludin and ZO-1 levels decreased within 6 h after the injection of LPS and were maximally decreased at 12 h after the induction of endotoxemia (Fig. 5A). By 18 h, NP-40-insoluble occludin and ZO-1 levels had begun to return toward normal. Total extractable ZO-2 and ZO-3 levels also decreased (Fig. 5B), and the observed changes in the expression of these proteins were similar, both with regard to kinetics and magnitude, to the observed changes in the expression of ZO-1 and occludin. As assessed by direct immunofluorescence, ZO-1 was localized in lung tissue from control mice as a continuous line along the boundaries between neighboring bronchial and alveolar epithelial cells (Fig. 6). The intensity of this staining was dramatically reduced in lung tissue harvested from mice that were challenged with LPS 12 h earlier (Fig. 6).
|
|
Pharmacological inhibition of iNOS activity ameliorates deranged TJ protein expression and targeting. Treating endotoxemic mice with L-NIL modulated the decrease in ZO-1 and occludin levels in NP-40-insoluble complexes (Fig. 7). Treatment with L-NIL failed to completely normalize levels of these proteins. Similarly, L-NIL treatment tended to preserve the normal ZO-1 staining pattern in lung tissue from mice exposed to LPS, but the staining pattern remained different from that observed in control specimens (Fig. 6).
|
![]() |
DISCUSSION |
---|
![]() ![]() ![]() ![]() ![]() ![]() |
---|
Herein, we showed that incubating Calu-3 pulmonary epithelial cell monolayers with a cocktail of proinflammatory cytokines (i.e., cytomix) markedly increased permeability to FD4. We also showed that injecting mice with LPS to induce systemic inflammation increased the leakage of FD4 from the blood compartment into the alveolar space. An increase in the BALF:serum FD4 ratio could be indicative of derangements in pulmonary endothelial or pulmonary epithelial barrier function or some combination of the two. However, our in vitro studies using Calu-3 bronchiolar-like epithelial cells support the view that an inflammatory milieu (produced in vitro by adding cytomix or produced in vivo by injecting LPS) increases the permeability of the pulmonary epithelial barrier. It is noteworthy that we were unable to clearly document an increase in the BALF:serum FITC-albumin ratio after the injection of mice with LPS. Because the pulmonary epithelium represents the major barrier to the movement of proteins like albumin (20) and horseradish peroxidase (43) from the blood compartment into the pulmonary air spaces (or vice versa), these results suggest that the magnitude of the inflammatory response in our murine model of acute endotoxemia was not sufficient to completely abolish the barrier provided by the epithelium. Further studies will be required to determine whether other components of TJs (e.g., claudins) remain properly assembled.
The magnitude of the functional alteration in pulmonary epithelial barrier function peaked at 12 h after the injection of LPS. By 18 h, the BALF:serum FD4 ratio was almost back to normal. This temporal pattern of changes in the barrier function of the bronchoalveolar epithelium was paralleled by changes in the expression of key proteins involved in the formation of TJs. For example, at 12 h after LPS injection, ZO-1 expression, as quantitated by immunoprecipitation and Western blotting, was virtually undetectable. However, at 18 h, a clear ZO-1 band was again apparent. The findings with respect to occludin and ZO-2 were similar.
Consistent with findings previously reported by Franek and colleagues (16), iNOS protein expression increased in total lung homogenates throughout the 18-h period of observation after injection of LPS. Nevertheless, the concentration of NO metabolites in BALF peaked at 12 h after the induction of endotoxemia and decreased at the 18-h time point. The discordance between iNOS protein levels in lung tissue and and
concentrations in BALF could be due to decreased enzymatic activity of iNOS or increased clearance of NO metabolites into the blood. In any event, however, we observed temporal associations between the concentration of NO metabolites in BALF on one hand and the functional changes in BALF and the expression of TJ proteins in the lung on the other hand. This temporal relationship suggests that the observed LPS-induced derangements in bronchoalveolar epithelial TJ structure and function were mediated in some way by increased local production of NO. This idea is further supported by the data we obtained using L-NIL to selectively inhibit iNOS enzymatic activity and thereby decrease NO biosynthesis. Treatment of mice with L-NIL ameliorated both the functional changes in pulmonary epithelial permeability induced by LPS and the changes in expression and localization of TJ proteins associated with endotoxemia.
The source(s) of NO in this animal model still needs to be determined. Others have demonstrated that rat alveolar and bronchial epithelial cells express iNOS after exposure to LPS (12). This finding suggests that the pulmonary epithelium, like the intestinal and hepatic epithelia, is a major source of NO in endotoxemia. However, Fujii et al. (17) showed that pretreating mice with gadolinium chloride, which depletes macrophages, decreases NO production and iNOS protein levels in endotoxemic mice. On the basis of these findings, these authors argued that infiltrating pulmonary macrophages were the major pulmonary source of iNOS and increased pulmonary NO biosynthesis in endotoxemic mice. An alternative explanation for the findings made by Fujii et al. can be articulated. Decreased production of iNOS in the lung in gadolinium chloride-treated animals could reflect decreased induction of iNOS in pulmonary epithelial cells as a result of a decreased production of proinflammatory cytokines by infiltrating or resident macrophages in the lung.
The mechanism(s) through which NO decreases the expression and interferes with the targeting of TJ proteins in pulmonary epithelial cells remains unknown. However, the results of some prior in vitro studies using Caco-2 human enterocyte-like epithelial cells suggest that the deleterious moiety is not NO per se, but rather ONOO-, a potent oxidizing and nitrating agent that is formed when NO reacts with the superoxide radical () (39). The permeability of Caco-2 monolayers increases when the cells are incubated with various NO donors, such as S-nitroso-N-acetylpenicillamine (SNAP) or sodium nitroprusside (35, 41). SNAP-induced hyperpermeability, however, is further augmented by the addition of diethyldithiocarbamate, a superoxide dismutase inhibitor, or pyrogallol, an
generator (35). Furthermore, SNAP-induced hyperpermeability is blocked by Tiron, an agent that scavenges
(35). SNAP-induced hyperpermeability is also prevented by various ONOO- scavengers, such as urate and deferoxamine (35). When Caco-2 monolayers are incubated with IFN-
or a combination of IFN-
, TNF-
, and IL-1
, iNOS expression is induced and permeability is increased (10, 47). The increase in permeability can be blocked by inhibiting NO production or scavenging ONOO- (10, 47). Collectively, these findings support the view that cytokine-induced intestinal epithelial hyperpermeability is mediated, at least in part, by the formation ONOO-.
Additional evidence can be mustered to support a role for ONOO- as a mediator of inflammation-induced lung epithelial hyperpermeability. The permeability of A549 human pulmonary epithelial monolayers increases after exposure to authentic ONOO- (46). Furthermore, in both experimental animals (23, 33) and humans (23, 30), acute pulmonary injury is associated with nitrotyrosine formation in the lung. Nitrotyrosine is a marker for the interaction of ONOO- (or other related reactive nitrogen species) with cellular proteins (39). Despite these data, further studies are required to determine whether ONOO- or some other reactive nitrogen intermediate is the actual moiety responsible for the deleterious effects of NO on TJ protein expression that we have observed in organs, including the lungs, of endotoxemic animals. Moreover, we can only speculate about the ways that ONOO- might induce alterations in the expression and localization of TJ proteins. It is reasonable, however, to hypothesize that highly reactive nitrogen species covalently modify amino acid residues in key proteins involved in regulating the synthesis and assembly of TJs (32). Conceivably, ONOO--mediated posttranslational events interfere with key signal transduction pathways or otherwise compromise the normal trafficking and interaction of proteins that are involved in the formation of TJs. Our laboratory is actively pursuing this line of investigation.
Acute lung injury and acute respiratory distress syndrome (ARDS) are common complications in critically ill patients. Considerable research has focused on endothelial dysfunction in the pathogenesis of pulmonary dysfunction. However, a relatively less studied component of the blood-air barrier is the alveolar epithelium, which plays an essential role in the clearance of fluid from the alveolar space (7). Alveolar fluid clearance is the result of ion gradients established, at least in part, by pumping Na+ across the basal membrane by Na+-K+-ATPase. The resulting ionic gradient results in passive movement of water through water channels in alveolar epithelial cells (14). Ware and Matthay (49) reported that alveolar fluid clearance is impaired in patients with acute lung injury and ARDS, and decreased alveolar fluid clearance is associated with extended mechanical ventilation and increased mortality. Our laboratory has obtained preliminary data indicating that Na+-K+-ATPase expression and activity are decreased in endotoxemic mice. Thus alveolar epithelial dysfunction is probably a significant component of the pathophysiology of pulmonary dysfunction in the critically ill patient. Decreased expression and function of TJ proteins in the alveolar epithelium would result in dissipation of ionic gradients and loss of motive force for the movement of water out of alveolar air spaces. Furthermore, the loss of the fence function of the TJ could also lead to a loss of the normal polarization of the alveolar epithelium into apical and basolateral domains and, therefore, derangements in transport function on this basis as well.
![]() |
ACKNOWLEDGMENTS |
---|
GRANTS
This work was supported by National Institute of General Medical Sciences Grants GM-58484 and GM-37631.
![]() |
FOOTNOTES |
---|
The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
![]() |
REFERENCES |
---|
![]() ![]() ![]() ![]() ![]() ![]() |
---|