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From the Division of Molecular and Cellular Biology,*
Department of Clinical Veterinary Science, University of Bristol,
Bristol, United Kingdom; the Institute for Medical Microbiology and
Immunology,
University of Ulm, Ulm, Germany;
and the Panum Institute,
University of
Copenhagen, Copenhagen, Denmark
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Abstract |
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 Top Abstract IntroductionMaterials and MethodsResultsDiscussionReferences |
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Introduction |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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Pathogenesis in these diseases reflects complex interactions between regulatory and effector mechanisms of various infiltrating and stromal cell populations. These include pro-inflammatory and anti-inflammatory cytokines, some of which, for example, transforming growth factor-ß (TGF-ß), may perform either function depending on the stage of the pathology.3 Also important are matrix proteinases, which facilitate lymphoid and myeloid cell infiltration, wound healing, and tissue remodeling4,5 but which may cause tissue destruction if unregulated. The particular combination of these elements operating in response to the initial stimulus will determine subsequent pathology.
Recent analyses of established IBD lesions suggest extracellular matrix proteolysis as a putative marker of disease progression in IBD. In particular, matrix metalloproteinases (MMPs) -9 and -3 have been associated with mucosal damage and fistulae in Crohn’s disease patients,6,7 MMPs 1, 3, and 13 with intestinal ulcer stroma, and MMPs 10 and 11 with the epithelium.8,9 Furthermore, CD4+ T cell activation in fetal intestinal explants equated with increased levels of MMP-1 and MMP-3, and exogenous MMP-3 promoted tissue degradation10 implying a causal role. Evidence of serine proteinases in IBD has been limited, with reports of undefined species associated with lesions from Crohn’s disease and ulcerative colitis patients,7,11 and in hapten-induced ulcerative lesions in rats.11
To evaluate therapies which mitigate unregulated tissue proteolysis, it is necessary to determine the role of specific proteinases at all stages of pathogenesis. This necessitates the use of model systems in which, like human disease, mucosal damage is a consequence of pathology rather than its cause.
When severe combined immunodeficient (SCID) mice are transplanted with
syngeneic or congenic CD4+ T cells the
transferred cells accumulate in mucosal tissues.12
In the
large intestine, these T cells proliferate, and induce colitis with
many of the features of human IBD.12-15
We have shown
that mucosal macrophage activation occurs early in the pathogenesis of
SCID colitis, along with tumor necrosis factor-
(TNF-) induction
in both macrophages and T cells,16
similar to human
Crohn’s disease.17,18
Subsequent up-regulation of TGF-ß
transcription occurs in established disease (Whiting, Williams,
Claesson, Reimann, and Bland, submitted).
It is known that TGF-ß promotes activation of plasminogen and other
serine proteinases,19
down-regulates many MMPs (although
not gelatinases), and promotes transcription of tissue inhibitors of
MMPs, whereas TNF- up-regulates most MMPs.20,21
The
potential for evaluating such changes in protease expression as a means
of monitoring normal tissue repair processes22,23
and
evaluating healing in chronic ulcers24
has been
demonstrated.
In this study, we have used the SCID mouse colitis model to define serine and metalloproteinase expression in established colitis, to localize proteinase activity within the tissue, and to co-localize with infiltrating and stromal cell types.
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Materials and Methods |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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Mice and Cell Transfer
C.B-17+/+ mice and congenic C.B-17scid/scid (SCID) mice were bred and housed under identical specific pathogen-free conditions. Experimental mice were injected intraperitoneally with 5 x 105 nonfractionated CD4+ splenic T cells and monitored for signs of disease, as previously described.25 Colonic tissue samples were taken at autopsy from eight CD4+ T cell-transplanted, diseased SCID, and two nontransplanted age- and sex-matched control SCID mice, 3 months after T cell transfer, and four C.B-17+/+ mice. Specimens from all mice were processed for gel and in situ zymographic analysis. Tissues were scored blind (0, no pathology to 3, severe pathology) for six disease parameters: tissue hypertrophy, CD3+ T cell infiltration, crypt hyperplasia, crypt distortion and branching, crypt abscesses, and ulceration.
Preparation of Tissue Samples
Colons were divided into three equal segments, distal, mid, and proximal. One centimeter from each was embedded in OCT (R. A. Lamb, London, UK) and snap-frozen in isopentane cooled over liquid nitrogen. Fecal material was removed from the remaining segments which were then flushed with 1 ml of phosphate-buffered saline, snap-frozen in liquid nitrogen, and stored at -80°C.
Specimens for biochemical analyses were pulverized to a powder using a freezer mill in liquid nitrogen, lyophilized, and the powder weighed. Brij 35 (0.1%) in triethanolamine (20 mmol/L) was added to the powder at 20 µl/mg and extraction performed for 16 hours at 4°C. Insoluble material was removed by centrifugation, and extracts mixed with nonreducing sodium dodecyl sulfate sample buffer. Uniform volumes were loaded for electrophoretic analyses, results therefore being normalized to original specimen dry weight.
Gelatin Substrate Sodium Dodecyl Sulfate-Polyacrylamide Gel Electrophoresis (Zymography)
Gelatin zymography was used to quantify MMP-2 and -9, as previously described.22 In brief, gelatin was co-polymerized in 10% polyacrylamide gels, and run in a Bio-Rad Mini Protean II apparatus (Bio-Rad, Hemel Hempstead, Herts, UK), with samples, prestained molecular weight markers (sodium dodecyl sulfate-7B), and MMP-2 standard (Biogenesis, Bournmouth, Dorset, UK). MMP proteolysis buffer was prepared from 50 mmol/L Tris/HCl, pH7.8, 50 mmol/L CaCl2, 0.5 mol/L NaCl, and 1 mmol/L amino phenyl mercuric acetate, with addition of a cocktail of serine proteinase inhibitors, comprising phenylmethyl sulfonyl fluoride (PMSF), leupeptin, and soybean trypsin inhibitor, at the concentrations detailed below. Gels were washed in 2.5% (v/v) Triton X-100 (BDH, Poole, Dorset, UK), incubated in the proteolysis buffer at 37°C for 18 hours, and stained with 0.2% Coomassie blue R250.
Casein Substrate Sodium Dodecyl Sulfate-Polyacrylamide Gel Electrophoresis (Zymography)
Casein zymography was used in the identification and quantitation of caseinolytic serine proteinases as previously described.24 In brief, 12.5% polyacrylamide gels were cast and run with Hammersten casein (BDH) as the substrate, and human neutrophil elastase, prepared from rheumatoid lung lavage,26 as enzyme standard. Rat neutrophil elastase, prepared from tissue from an excisional wound model,23 was also used for comparison. Proteolytic clarification of the electrophoresed gels was performed as appropriate for serine proteinases in 100 mmol/L phosphate buffer (pH 6.8) supplemented with 8 mmol/L ethylenediaminetetraacetic acid (EDTA) and 0.2% (v/v) Triton X-100.
Inhibition Studies
The proteinase class responsible for the clarified zones in each analysis was identified by incorporating, as appropriate: MMP inhibitors, EDTA (50 mmol/L, and omitting CaCl2), or peptidyl hydroxamate (1 µmol/L; Calbiochem, Nottingham, Notts, UK); serine proteinase inhibitors PMSF (1 mmol/L), or 4-(2-aminoethyl)-benzenesulfonyl fluoride hydrochloride (Pefabloc, 4 mmol/L; Boehringer Mannheim, Lewes, E. Sussex, UK); trypsin-like enzyme inhibitors, soybean trypsin inhibitor (20 µg/ml), or leupeptin (50 µmol/L); elastase inhibitor, elastatinal (50 µmol/L); or cysteine proteinase inhibitor trans-epoxysuccinyl-L-leucylamido(4-guanidino)-butane (E64, 25 µmol/L), in the proteolysis buffers. The identity of MMP-2 and -9 was further corroborated by demonstrating gelatin affinity, as previously described.22
Densitometric Analysis
Quantitative densitometry was performed as previously described.27,28
In Situ Zymography
Localization of active enzymes was performed by in situ zymography based on the method of Galis et al.29 Fluorescein isothiocyanate-casein (1 mg/ml) was dissolved in incubation buffer (50 mmol/L Tris-HCl, pH 7.5, 10 mmol/L CaCl2, 0.05% Brij 35), filtered, and spread on glass slides. After air-drying, substrate uniformity was confirmed by fluorescence microscopy. Frozen sections (8 µm) were transferred to substrate-coated slides (experimental and control specimens on the same slide), air-dried, and covered with incubation buffer and coverslip, secured with nail varnish. Slides were incubated at 37°C and 100% humidity, to allow substrate:label proteolysis, and monitored every 2 to 3 days. Control slides were incubated either at 4°C, or at 37°C in the presence of appropriate proteinase inhibitors. Released fluorescein was washed from beneath the coverslip with incubation buffer. Areas of active enzyme were identified by clearance of labeled substrate.
To characterize the nature of the active proteinases involved in substrate degradation, EDTA (20 mmol/L), peptidyl hydroxymate MMP inhibitor (10 µmol/L), aprotinin (50 µg/ml), soybean trypsin inhibitor (100 µg/ml), PMSF (1 mmol/L), pepstatin (1 µmol/L), or E64 (25 µmol/L), were added at the start of incubation and replenished every 2 to 3 days.
Immunohistochemistry, Antibodies, and Reagents
Immunohistochemistry was performed as previously described,16 using rat monoclonal antibodies raised against CD3 (clone KT3; Serotec, Oxford, UK), mouse macrophage (clone A3–1, F4/80 antigen; Serotec), mouse activated macrophage (clone 158.2, ATCC, HB8466), and mouse CD11b (M1/70; Serotec). Secondary antibody was biotin-conjugated goat anti-rat IgG (Harlan Sera-Lab, Loughborough, Leics, UK). StreptABComplex/HRP peroxidase complex (DAKO A/S, Glostrup, Denmark), and diaminobenzidine-4HCl, was used to visualize the staining.
Statistical Analysis
The Mann-Whitney U test of the quantitative zymography data were performed using the Genstat statistics package. A P value of 0.05 or less was regarded as significant. In all plots, means and standard errors are shown.
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Results |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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Tissues from eight diseased SCID mice, two nontransplanted SCID
mice, and four C.B-17+/+ mice were stained for
CD3 to determine levels of T cell infiltration, or for CD11b to assess
polymorph infiltration and the development of crypt abscesses. At least
two sections from proximal, mid, and distal colon tissues from each
mouse were scored in a blinded manner for pathological changes. The
results are presented in Table 1
.
Pathology ranged from mild (mouse 3) to severe (mouse 8), and was in
accordance with previous findings.30
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There was a clear up-regulation in serine proteinase activities in
the colitic mice specimens (Figure 1, A and D)
, the majority of which displayed substantial levels of serine
caseinolytic activity, whereas only one C.B-17+/+
sample, and no nontransplanted SCID samples, showed comparable activity
(Figure 1, B and D)
.
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demonstrated significantly higher
levels of total serine proteinase activity in the transplanted SCID
samples compared with nontransplanted SCID (P <
0.01) and C.B-17+/+ (P =
0.01) control mice. The major species were 45-kd, 23-kd, and 30-kd
proteinases. Levels of each of these proteinases were elevated in the
transplanted SCID mice, compared with negligible levels in the SCID
controls (45 kd, P < 0.01; 30 kd, P =
0.03; 23 kd P < 0.01), and intermediate levels in
C.B-17+/+ mice (45 kd, P = 0.04;
30 kd, P = 0.03; 23 kd P < 0.01).
In those mice with high levels of serine proteinases, expression was
generally greatest in the proximal colon samples (Figure 1E)
. Total
serine proteinase activity in the IBD mice increased eightfold between
the distal and proximal regions (P < 0.01),
fourfold for the 45-kd proteinase (P < 0.01),
10-fold for the 30-kd species (P < 0.01), and
sixfold for the 23-kd proteinase (P < 0.01).
A 23-kd serine proteinase was found in the colon lumen contents of all mice, elevated in IBD compared with C.B-17+/+ and SCID controls, and was evident throughout the small intestinal lumen (data not shown). However, there was no evidence of either the 45-kd or 30-kd proteinase in the lumen.
Inhibition with leupeptin, soybean trypsin inhibitor, and PMSF demonstrated that the three major species were trypsin-like serine proteinases. Co-migration of the 30-kd species with rat neutrophil elastase, and its inhibition by elastatinal (data not shown), indicate this proteinase to be neutrophil elastase.
Analysis of pancreatic extracts demonstrated strong bands at 23 and 25
kd corresponding to trypsin and chymotrypsin, respectively, according
to comparisons with standards, and at 45 kd (Figure 1C)
. The trypsin
co-migrated with the 23-kd protease found in colitic tissue and gut
lumen, and the 45-kd band with that found in colitic tissue, implying
identity in each case. However, there was no clear evidence of species
corresponding with chymotrypsin in colitic tissue, or neutrophil
elastase in the pancreatic samples.
Immunoblotting studies using antiserum to plasmin/plasminogen indicated that the 45-kd proteinase was not plasmin (data not shown).
MMPs Were Up-Regulated and Activated in Colitis
Quantitative zymography demonstrated a marginal decrease in the
level of proMMP-2 in IBD samples, as compared with the SCID
(P = 0.06) and C.B-17+/+
(P = 0.24) control samples (Figure 2, A–C)
. However, this may be because of
conversion to the activated form, which occurred
(P < 0.03) in the IBD samples (Figure 2D)
.
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, with respect to both control groups (P
< 0.01), and the activated forms of MMP-9, absent in all of the
control specimens, were also evident in colitis
(P < 0.01). In two of the transplanted SCID
samples (no. 2 proximal and no. 8 distal) a 130-kd
neutrophil-associated complex between MMP-9 and
lipocalin22,31
was identified.
Regional differences in colon MMP expression (Figure 2E)
were not as
marked as with the serine proteinases. There was a trend for pro-
(P = 0.01) and active (P
= 0.14) MMP-9 and active MMP-2 (P = 0.01) to
decrease proximal to distal in the colitic colons. There was no
apparent regional variation in the levels of proMMP-2
(P = 0.6).
Some colitic samples were generally more proteolytically active than others, and hence there was a correspondence between levels of different protease species in these samples. Correlations ranged from r = 0.285 (not significant) for activated MMP-9 and the 30-kd serine protease, to r = 0.871 (P < 0.001) for pancreatic trypsin and the 45-kd serine protease. A very good correspondence was seen between MMP-2 activation and total serine protease levels (r = 0.824, P < 0.001), and more particularly with pancreatic trypsin (r = 0.817, P < 0.001). This suggests a relationship between serine protease penetration into gut tissue and resident MMP activation.
MMPs Are Activated by Fecal Proteases, but not during Extraction
Experiments were performed to investigate the potential for gut lumen-derived proteases to activate tissue MMPs. Firstly, under conditions prevailing during extraction, the potential influence of fecal contamination on the apparent tissue levels of activated MMPs was determined. Secondly, the potential for luminal proteases to activate MMPs within the tissue was evaluated, by incubating under conditions appropriate for proteolysis.
Mouse gut luminal contents were titrated, and monitored by casein zymography, to equalize protease levels present during incubations to those identified in colitic tissues. Human acute wound fluid, containing proMMP-9 and proMMP-2, but no activated gelatinases22 was incubated for 16 hours at 4°C, in accordance with the extraction procedure, or at 37°C in proteolysis buffer. Control incubations were performed using fecal extract alone, wound fluid alone, or wound fluid with lumen contents and soybean trypsin inhibitor and Pefabloc to inactivate serine proteases. Trypsin and chymotrypsin were each titrated to estimate levels found in colitic tissue, as for the fecal extracts, and appropriate levels incubated with wound fluids, as above. All experiments were performed in triplicate.
Under extraction conditions, no activation of wound fluid MMP-9 or
MMP-2 was seen with the fecal extracts (Figure 3A)
. However, at 37°C, under conditions
appropriate for proteolysis, degradative processing of proMMP-9 and
proMMP-2 was apparent, in particular, generating a
Mr 75-kd-activated form of MMP-9 seen in colitic
tissue (Figure 2A)
. Treatment of wound fluids with trypsin, even under
extraction conditions, resulted in processing of MMP-2 and -9 (Figure 3B)
. At 37°C all proMMP-9 was converted to the
Mr 75-kd-activated form, and all proMMP-2 was
lost, with the appearance of species at Mr 52 and
38 kd. Incubation of the wound fluids with chymotrypsin generated a
Mr 80-kd-activated form of MMP-9 which was not
seen in the fecal extract incubation, but was seen in colitic tissue,
and resulted in processing of proMMP-2 (Figure 3C)
. Wound fluid alone
did not generate any activated species either in extraction buffer at
4°C (Figure 3D)
, or under conditions appropriate for proteolysis. No
MMPs were identified in the fecal extracts (data not shown).
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In control tissue, low levels of proteinase activity were
localized by in situ zymography to normal colonic epithelium
of C.B-17+/+, nontransplanted SCID and apparently
unaffected colon of transplanted SCID mice. This proteolysis was
associated with the luminal epithelium, rather than that of the lower
crypt (Figure 4A)
. Proteolysis associated
with lymphoid tissue of control colons was observed in mucosal lymphoid
follicles of C.B-17+/+ mice (Figure 4B)
, but no
proteolysis was localized to the occasional, presumably pre-B cell,
lymphoid aggregates of SCID mice (Figure 4C)
. In diseased mice,
degradation was particularly marked in areas of epithelium overlying
heavily infiltrated regions of mucosa and within the infiltrated lamina
propria (Figure 4D)
. In the deeper layers of inflamed mucosa there was
evidence for extensive proteolytic activity within the epithelium and
as a subepithelial sheath within the lamina propria (Figure 4F)
.
Inhibitor studies showed that this was due more to the action of MMPs
than of serine proteases (Figure 4, G and H)
, and that neither cysteine
nor aspartic proteinases seemed to contribute (not shown). Consecutive
sections of the heavily infiltrated regions, treated for in
situ zymography and immunohistochemistry, showed that they
comprised CD3+ T cells,
CD11b+ myeloid cells, and activated macrophages
(Figure 5, C–F)
. Immediately subjacent
to the epithelial cell basement membrane
CD11b+/F4/80- cells,
probably neutrophils, were the most abundant cell type (Figure 5D)
.
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Discussion |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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There have been few previous reports of serine proteinases in intestinal inflammation. In human colitis and Dinitrobenzenesulfonic acid-induced colitis in the rat, Hawkins et al11 showed increases in total serine proteinase activity in diseased colonic tissue similar to those demonstrated here, and identified the same predominant 45- and 23-kd species. Similarly, Baugh et al7 demonstrated 45-kd and 23-kd gelatinolytic proteases inhibitable by aprotinin, a serine protease inhibitor. Interestingly, the 45-kd species has also been detected in normal human colon, but only after trypsin activation. Our studies in the mouse model show a clear correlation between total serine protease, and trypsin in particular, and MMP activation. Experiments demonstrated that MMP activation was not because of exposure to contaminating luminal serine proteases during the extraction procedure, but did occur when MMPs were exposed to luminal proteases under near physiological conditions. This implies that, at least in advanced colitis, tissue proteases are accessible for activation by luminal proteases through a defective epithelial barrier, even in the absence of frank ulceration, and that activation of tissue proteases by luminal proteases may play a role in pathogenesis. Detection of neutrophil elastase in the mouse model conforms with established characteristics of colitis, and fecal elastase has been proposed as a marker in ulcerative colitis,32 and a target for therapy.33 Neutrophil involvement in the model ranged from local foci in the colonic mucosa of mild inflammation, to significant and widespread accumulations, notably in crypt abscesses and the lumen. In a few colitic samples, a 130-kd MMP-9/lipocalin complex, associated with neutrophil infiltrations31 was evident. This implies that the elastase detected in zymograms in this study reflects tissue neutrophilia, a view corroborated by serial immunohistochemistry and in situ zymography.
In colitic tissue specimens, elevated serine proteinase expression was associated with processing of MMPs, with the appearance of activated forms of MMP-9 (80 and 75 kd) and MMP-2 (58 and 45 kd), and ultimately their complete degradation. Although the overall levels of MMP-2 did not alter as a correlate of disease, the proportion identified in the active form increased considerably and significantly. MMP activation was clearly correlated with serine proteinase activity, comparable to the widespread MMP activation seen in chronic dermal ulcers, also associated with extracellular serine proteinase.24 Considering the central role plasmin has in the physiological cascade of events leading to MMP activation,34 this was deemed a candidate for the identity of the uncharacterized serine protease in our studies. However, we were unable to confirm the presence of plasmin in the inflamed tissue. Increased MMP-9 and unchanged MMP-2 expression corroborated the findings of a previous immunohistochemical study,6 which was unable to distinguish pro- and activated forms. The recent work of Baugh et al7 clearly shows that MMP-9 is a major factor in human intestinal inflammation, and was assumed to be a product of neutrophilia. Our results also show spatial correlations between MMP-9 activation, neutrophil accumulation, and tissue damage, although low levels of the lipocalin complex implies that other cell types may be expressing this protease.
MMP-1 (interstitial collagenase) and MMP-3 (stromelysin-1), probably
derived from fibroblasts and macrophages, respectively, have been
implicated in tissue destruction in Crohn’s disease,9
although these in situ hybridization studies provide no
information on enzyme expression or activation. It has also been shown
that MMP-3, probably stimulated by T-cell-derived TNF-, contributes
to tissue degradation10,35
in a system involving mucosal T
cell activation in human fetal explants. This early T-cell-mediated
MMP-3 induction has primarily been superseded in our model by
inflammation and repair. Also, this explant model does not take account
of the extensive myeloid cell infiltration seen in the mouse and,
frequently, in human disease, with associated increase in neutrophil
elastase and MMP-9, identified in this study and in human
disease.7
It may also be that the initial TNF-
induction of MMP-3 has been superseded by TGF-ß induction of MMP-9 in
advanced pathology.21,36
This study clearly shows
gelatinolytic activity in pericryptal stroma of diseased tissue in the
region of the activated myofibroblast sheath, which displays increased
TGF-ß receptor expression in the mouse model (work in
progress). Proteolytic activity facilitating inflammatory infiltration
may lead to more extensive matrix degradation as a result of the
inappropriate activation events indicated in this study. Furthermore,
proteolysis localized to the epithelium overlying areas of intense
infiltration was of particular interest, as it may promote damage to
the epithelial barrier. The activity observed resulted from both serine
proteinases and MMPs, and was associated with activated macrophages and
neutrophils. Macrophages transcribing metalloelastase (MMP-12) have
been identified close to shedding mucosal epithelium in ulcerative
colitis and Crohn’s disease,8
and matrilysin
(MMP-7)37
has been noted in IBD epithelium, especially
adjacent to crypt abscesses, and associated with basement membrane
degradation.9
The clear and significant bias toward higher regional proteinase activity in proximal colon is somewhat at odds with clinical presentation in human disease. This may result from variable distribution of initiating T cells, inflammatory cell infiltration, luminal antigens, protease inhibitors, or the nature of the epithelial barrier, and needs further investigation. In severe disease regional distinctions were mitigated, with high levels detected throughout the colon (data not shown).
The acute inflammatory state normally represents a transient, co-ordinated proteolytic episode which gives way to phases of remodeling and tissue regeneration. Persistence of inflammation may be due to a loss in co-ordination of degradative and reparative processes, maintenance of pro-inflammatory elements, such as infection or activation of cytokines, or the introduction of elements that promote tissue destruction. Colonic tissue, even under normal circumstances, is a site of active proteolysis associated with digestive processes and continual turnover of the epithelium. It is postulated here that, at some stage during the initial inflammatory episode, other factors shift the balance of turnover in favor of proteolysis resulting in tissue damage, thus preventing regeneration and the resolution of inflammation. These factors may include tissue proteolysis resulting from inappropriate penetration of luminal enzymes, widespread activation of MMPs associated with inflammation, or the excessive potentiation of cytokines. Furthermore, these factors are likely to interact in a cascade of events resulting in positive feedback and progressive deterioration. Thus, what begins as an inflammatory episode becomes a disorder of combined connective tissue and inflammatory pathologies. Importantly, this model will permit dissection of the sequence of events from initial T cell infiltration and proliferation, through infiltration by other cell types, to subsequent tissue damage and fibrosis.
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Footnotes |
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Supported by the European Union Research Contract Numbers BMH4-96-0612, QLGI-1999-00050.
Accepted for publication August 21, 2000.
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References |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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, whereas ulcerative colitis LP cells manifest increased secretion of IL-5. J Immunol 1996, 157:1261-1270[Abstract]
ß (+) T-cells in the pathogenesis of murine inflammatory bowel-disease. Eur J Immunol 1994, 24:2803-2812[Medline]
ß T cells in the colonic lamina propria of scid mice with colitis. Eur J Immunol 1996, 26:1156-1163[Medline]
(TNF-) transcription and translation in the CD4(+) T cell-transplanted scid mouse model of colitis. Clin Exp Immunol 1999, 116:415-424[Medline]
and interferon- production measured at the single cell level in normal and inflamed human intestine. Clin Exp Immunol 1990, 81:301-305[Medline]
in childhood chronic inflammatory bowel-disease. Gut 1991, 32:913-917ß T cells in SCID mice, with colitis. Eur J Immunol 1996, 26:3074-3083[Medline]
and interleukin 10 in adult respiratory distress syndrome. Thorax 1997, 52:442-446[Abstract]
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C. V. Whiting, J. F. Tarlton, M. Bailey, C. L. Morgan, and P. W. Bland Abnormal Mucosal Extracellular Matrix Deposition Is Associated with Increased TGF-{beta} Receptor-expressing Mesenchymal Cells in a Mouse Model of Colitis J. Histochem. Cytochem., September 1, 2003; 51(9): 1177 - 1189. [Abstract] [Full Text] [PDF]
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O. R.F. Mook, C. Van Overbeek, E. G. Ackema, F. Van Maldegem, and W. M. Frederiks In Situ Localization of Gelatinolytic Activity in the Extracellular Matrix of Metastases of Colon Cancer in Rat Liver Using Quenched Fluorogenic DQ-gelatin J. Histochem. Cytochem., June 1, 2003; 51(6): 821 - 829. [Abstract] [Full Text] [PDF]
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N. Cenac, A.-M. Coelho, C. Nguyen, S. Compton, P. Andrade-Gordon, W. K. MacNaughton, J. L. Wallace, M. D. Hollenberg, N. W. Bunnett, R. Garcia-Villar, et al. Induction of Intestinal Inflammation in Mouse by Activation of Proteinase-Activated Receptor-2 Am. J. Pathol., November 1, 2002; 161(5): 1903 - 1915. [Abstract] [Full Text] [PDF]
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J. R. Allport, Y.-C. Lim, J. M. Shipley, R. M. Senior, S. D. Shapiro, N. Matsuyoshi, D. Vestweber, and F. W. Luscinskas Neutrophils from MMP-9- or neutrophil elastase-deficient mice show no defect in transendothelial migration under flow in vitro J. Leukoc. Biol., May 1, 2002; 71(5): 821 - 828. [Abstract] [Full Text] [PDF]
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