2 Facultad de Ciencias, Universidad Nacional Autonoma de Mexico, Coyocán México DF CP 04000; 1 Instituto Nacional de Enfermedades Respiratorias, México DF CP 14080, Mexico; and 3 Department of Pathology, Baylor College of Medicine, Houston, Texas 77030
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ABSTRACT |
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Fibroblast proliferation and extracellular matrix accumulation characterize idiopathic pulmonary fibrosis (IPF). We evaluated the presence of tissue inhibitor of metalloproteinase (TIMP)-1, -2, -3, and -4; collagenase-1, -2, and -3; gelatinases A and B; and membrane type 1 matrix metalloproteinase (MMP) in 12 IPF and 6 control lungs. TIMP-1 was found in interstitial macrophages and TIMP-2 in fibroblast foci. TIMP-3 revealed an intense staining mainly decorating the elastic lamina in vessels. TIMP-4 was expressed in IPF lungs by epithelial and plasma cells. TIMP-2 colocalized with Ki67 in fibroblasts, whereas TIMP-3 colocalized with p27 in inflammatory and epithelial cells. Collagenase-1 was localized in macrophages and alveolar epithelial cells, collagenase-2 was localized in a few neutrophils, and collagenase-3 was not detected. MMP-9 was found in neutrophils and subepithelial myofibroblasts. Myofibroblast expression of MMP-9 was corroborated in vitro by RT-PCR. MMP-2 was noticed in myofibroblasts, some of them close to areas of basement membrane disruption, and membrane type 1 MMP was noticed in interstitial macrophages. These findings suggest that in IPF there is higher expression of TIMPs compared with collagenases, supporting the hypothesis that a nondegrading fibrillar collagen microenvironment is prevailing.
tissue inhibitor of metalloproteinases; gelatinases; collagenase; fibrosis
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INTRODUCTION |
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IDIOPATHIC PULMONARY FIBROSIS (IPF) is a progressive and usually lethal interstitial lung disease of unknown etiology characterized by varying degrees of inflammation and fibrosis in the lung parenchyma (14).
The fibrotic response is generally considered an irreversible process and is characterized by a striking increase in fibroblast population and a profound and complex change in extracellular matrix (ECM) turnover. That brings about a progressive accumulation of connective tissue proteins (5) and, in addition, basement membrane disruption that is observed mainly in the early stages of the disease (25). In this context, an imbalance between the synthesis and degradation of ECM molecules in the local lung microenvironment appears to be of central importance in the pathogenesis of the fibrotic component of IPF.
Matrix metalloproteinases (MMPs), the mediators of matrix degradation, are a family of zinc endoproteinases that share structural domains and are collectively capable of degrading essentially all ECM components (2). At present, the human MMP gene family contains 17 members that can be divided by structure and substrate specificity into several subgroups including collagenases, gelatinases, stromelysins, and membrane-type (MT) MMPs; other MMPs do not appear to fall into any of these subgroups (36, 37). The regulation of these enzymes reveals similarities and differences. They differ in cellular sources and inducibility, but they share the property of being synthesized as inactive zymogens in which activation can occur through intracellular, extracellular, or cell surface-mediated proteolytic mechanisms (2, 26, 37).
A pivotal extracellular control of MMP catalytic activity is accomplished by members of a specific family of inhibitors named tissue inhibitors of metalloproteinases (TIMPs). There are currently four members of the TIMP family (TIMP-1 to -4) that, besides their common MMP inhibitory action, differ in expression patterns and other properties such as association with latent MMPs, cell growth-promoting activity, cell survival-promoting activity, and apoptosis (1, 7, 9).
The possible role of both MMPs and TIMPs in IPF is at present unclear. It has been considered that TIMPs are good candidates for tissue fibrosis, but studies in lung fibrosis are scanty. There are two recent studies (6, 11) exploring the localization of TIMP-2, and in one of them (11), TIMP-1 was also evaluated. However, the expression and localization of TIMP-3 and TIMP-4 have not been examined in any fibrotic lung disorder.
The aim of this study was to determine the localization of TIMP-1, TIMP-2, TIMP-3, and TIMP-4 in lung tissue obtained from patients with IPF. Additionally, we colocalized TIMP-2 and TIMP-3, which have been related with cell growth-promoting activity and apoptosis, respectively (1, 10), with the nuclear proteins Ki67 (associated with proliferation) and p27 (inhibitor of the cell cycle). To have a more integrated picture of matrix remodeling, we also examined a variety of MMPs including the collagenase subfamily (MMP-1, MMP-8, and MMP-13), the gelatinase subfamily (MMP-2 and MMP-9), and MT1-MMP.
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MATERIALS AND METHODS |
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Study population. Twelve nonsmoking patients with IPF were included in this study (8 men and 4 women; mean age 58.1 ± 13.2 yr). The protocol was approved by the Ethical Committee of the Instituto Nacional de Enfermedades Respiratorias (Mexico DF, Mexico). Diagnosis of IPF was supported by clinical, radiological, computed tomography scan, and functional findings of interstitial lung disease and was corroborated by open lung biopsy (22, 27). The morphological diagnosis of IPF was based on typical microscopic findings and included patchy, nonuniform alveolar septal fibrosis and interstitial inflammation consisting mostly of mononuclear cells but also of neutrophils and eosinophils; a variable macrophage accumulation was observed in the alveolar spaces as was the cuboidalization of the alveolar epithelium. Biopsies lacked granulomas, vasculitis, microorganisms, and inorganic material as seen by polarized light microscopy. None of the patients had been treated with steroids or other immunosuppressive drugs at the time of biopsy. As controls, histologically normal lung tissues obtained at necropsy from six nonsmoking adult individuals (4 men and 2 women; mean age 43.2 ± 11.1 yr) who died of causes unrelated to lung diseases were utilized.
Bronchoalveolar lavage.
Bronchoalveolar lavage (BAL) was performed with a standard technique
(32). Briefly, the fiber-optic bronchoscope was wedged in
two separate segments of the right middle lobe or lingula, and 300 ml
of normal saline were instilled in 50-ml aliquots, with an average
return of 70%. The recovered BAL fluid was filtered through sterile
gauze, measured, and then centrifuged at 250 g for 10 min at
4°C. The supernatants were kept frozen at 70°C until used. The
cell pellet was resuspended in 1 ml of phosphate-buffered saline (PBS),
and an aliquot was used to evaluate the total number of cells. Other
aliquots were fixed in carbowax, and three slides per sample were
stained with hematoxylin and eosin, Giemsa, and toluidine blue and used
for differential cell counts. Six nonsmoking healthy volunteers were
lavaged as control subjects (3 women and 3 men; 33.5 ± 6 yr old).
Immunohistochemistry. Tissue sections were deparaffinized, rehydrated, and then blocked with 0.45% H2O2 in methanol for 30 min followed by normal serum (Vector Laboratories, Burlingame, CA) diluted 1:20 in PBS for 20 min. Before the immune reaction, antigen retrieval with 0.1 M citrate buffer, pH 6.0, was performed. The sources of the primary monoclonal antibodies were Fuji Chemical Industries (Toyama, Japan) for MMP-1, MMP-8, MMP-9, MMP-13, TIMP-1, TIMP-2, and TIMP-3 and Calbiochem (San Diego, CA) for MMP-2. TIMP-4 polyclonal antibody was kindly donated by S. S. Apte (Cleveland Clinic Foundation, Cleveland, OH). The monoclonal antibody for mitotic inhibitor/suppressor protein p27 was from NeoMarkers (Fremont, CA), and Ki67 rabbit polyclonal antibody was from Novocastra Laboratory (Newcastle, UK). Antibodies were applied and incubated at 4°C overnight. A secondary biotinylated anti-immunoglobulin followed by horseradish peroxidase-conjugated streptavidin (BioGenex, San Ramon, CA) was used according to the manufacturer's instructions. 3-Amino-9-ethylcarbazole (BioGenex) in acetate buffer containing 0.05% H2O2 was used as the substrate. The sections were counterstained with hematoxylin (19). The primary antibody was replaced by nonimmune serum for negative control slides.
To identify epithelial cells, myofibroblasts, and macrophages, parallel sections were immunostained for cytokeratin 7,Evaluation of immunohistochemical results. The intensity of the staining in different lung tissue components was evaluated in the IPF patients as described previously (11). A scale from 0 to 3 was used as follows: 0, negative; 1, mild staining; 2, moderate staining; and 3, strong staining.
In situ hybridization. Riboprobes for in situ hybridization were generated from human cDNA TIMP-4 cloned in a pGem-T vector provided by S. S. Apte (Cleveland Clinic Foundation). The plasmid was linearized before translation with Kpn I. An antisense 487-bp fragment was transcribed with T7 and a sense 508-bp fragment with SP6 RNA polymerase, respectively. The transcription of sense and antisense transcripts was performed with a labeling mixture containing digoxigenin-UTP (Boehringer Mannheim, Mannheim, Germany).
In situ hybridization was performed on 4-µm sections as previously described (19). Briefly, the sections mounted on silanized slides were incubated in 0.001% proteinase K (Sigma, St. Louis, MO) for 20 min at 37°C. After acetylation with acetic anhydride, the sections were prehybridized for 1 h at 45°C in a hybridization buffer. The sections were incubated with the digoxigenin-labeled probes at 45°C overnight. Some sections were hybridized with a digoxigenin-labeled sense RNA probe. The tissues were incubated with a polyclonal sheep anti-digoxigenin antibody coupled to alkaline phosphatase (Boehringer Mannheim, Indianapolis, IN) for 1 h at room temperature. The color reaction was performed by incubation with Fast Red chromogen (Biomeda). The sections were lightly counterstained with hematoxylin.Fibroblast isolation and culture. Human fibroblast-like cells were obtained from normal and IPF lungs as previously described (20). Cells were isolated by trypsin dispersion and grown in Ham's F-12 medium (GIBCO BRL, Life Technologies, Grand Island, NY) supplemented with 10% fetal calf serum. The cells were cultured at 37°C in 5% CO2-95% air in 25-cm2 Falcon flasks with F-12K medium (GIBCO BRL) supplemented with 10% fetal bovine serum (GIBCO BRL), 100 U/ml of penicillin, and 100 µg/ml of streptomycin. When the fibroblasts reached early confluence, the medium was replaced with serum-free F-12K medium containing phorbol 12-myristate 13-acetate (PMA). Fibroblasts were collected for RNA extraction.
Flow cytometry.
In parallel experiments, fibroblasts were fixed with ice-cold 70%
ethanol and stored at 20°C until assayed. The cells were washed and
incubated for 1 h at 37°C with FITC-conjugated monoclonal anti-human
-smooth muscle actin antibody diluted 1:400 in 1% bovine
serum albumin in PBS, pH 7.3. The fibroblasts were washed and
resuspended in PBS for fluorescence-activated cell sorter analysis as
described elsewhere (35).
Zymography. SDS-polyacrylamide gels containing gelatin (1 mg/ml) were used to identify proteins with gelatinolytic activity from BAL supernatants (21). After electrophoresis, the gels were washed in a solution of 2.5% Triton X-100 (15 × 2 min) to remove SDS, washed extensively with water, and incubated overnight at 37oC in 100 mM glycine, pH 7.6, containing 10 mM CaCl2 and 50 nM ZnCl2. Identical gels were incubated in the presence of 20 mM EDTA as controls. The gels were stained with Coomassie brilliant blue R250 and destained in a solution of 7.5% acetic acid and 5% methanol.
RT-PCR. Total RNA extracted from human fibroblasts as previously described (20) was used for RT-PCR to explore gelatinase B expression. Total RNA extracted from IPF and control lungs was used to analyze MMP-13 and TIMP-4 expression. RNA was reverse transcribed to synthesize cDNA according to the manufacturer's protocol (GIBCO BRL).
PCR amplification (Perkin-Elmer 9600, Branchburg, NJ) for glyceraldehyde-3-phosphate dehydrogenase (GAPDH), MMP-9, MMP-13, and TIMP-4 was performed with a cDNA working mixture in a 25-µl reaction volume containing 20 mM Tris · HCl, pH 8.3, 50 mM KCl, 2 mM MgCl2, 200 µM deoxynucleotide triphosphates, 1 µM specific 5' and 3' primers, and 1 U of Taq DNA polymerase (Perkin-Elmer). The set of primers used for the GAPDH PCR was 5'-CATCCATCCCGTGACCTTAT-3' and 5'-GCATGACTCTCACAATGCGA-3', with an amplified product of 395 bp. Nucleotides 5'-TCATGACCTCATCTTC-3' and 5'-GAACAGCTGCACTTAT-3' were used as primers to amplify a 134-bp segment for collagenase-3 cDNA. For TIMP-4 amplification, the primers used were 5'-CCAGAGGTCAGGTGGTAA-3' (antisense) and 5'-ACAGCCAGAAGCAGTATC-3' (sense) for a fragment size of 446 bp. Gelatinase B primers were 5'-GTCGGCCTCAAAGGTTTGGAAT-3' (antisense) and 5'-GTGCTGGGCTGCTGCTTTGCTG-3' (sense), with an amplified product of 303 bp. To quantify the housekeeping gene GAPDH, a competitor was constructed by cutting an internal fragment of 155 bp of a GAPDH cDNA (originally 1,233 bp) cloned in a PBR 322 plasmid with Nco I. The modified GAPDH cDNA was subsequently religated. The competitor (cGAPDH) sequence was obtained by PCR amplification of the modified plasmid with the primers for GAPDH. The competitor size was 240 bp. Fourfold serial dilutions of the standard competitor (5, 10, 15, and 20 pg) were coamplified with a constant amount of cellular cDNA (1 µl). Cycling conditions were 95°C for 10 min for 1 cycle; 95°C for 30 s, 58°C for 30 s, and 72°C for 120 s for 40 cycles; and 72°C for 7 min for the final incubation. Aliquots (5 µl) of the PCR product were resolved in 1.5% agarose gel containing ethidium bromide. Band intensities were quantitated by scanning densitometry with a Kodak digital science electrophoresis documentation and analysis system 120 (Kodak, Rochester, NY). The logarithm of the GAPDH-to-cGAPDH ratio was plotted as a function of the logarithm of the known cGAPDH amount. The point of equivalence represents the concentration of GAPDH in the cDNA sample. Dilutions were performed to reach 5 pg/µl of GAPDH. For each amplification, 10 pg of GAPDH were used. For MMP-13 and gelatinase B amplification, cycling conditions were 95°C for 10 min for 1 cycle; 95°C for 30 s, 60°C for 30 s, and 72°C for 90 s for 35 cycles; and 72°C for 7 min for the final incubation. For TIMP-4 amplification, the conditions were 95°C for 10 min for 1 cycle; 95°C for 30 s, 58°C for 30 s, and 72°C for 60 s for 38 cycles; and 72°C for 7 min for the final incubation. Aliquots (5 µl) of the PCR product were resolved on a 1.5% agarose gel containing ethidium bromide. ![]() |
RESULTS |
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TIMP-1, TIMP-2, TIMP-3, and TIMP-4 localization.
TIMP-1 was detected in 8 of 12 IPF lungs, usually localized in isolated
interstitial cells, mainly macrophages and fibroblast-like cells (Fig.
1, A and B). This
inhibitor was observed in areas of dense scar tissue.
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RT-PCR for TIMP-4 mRNA.
Expression of TIMP-4 in two IPF lungs and two control lungs was
analyzed by RT-PCR. As illustrated in Fig.
4, the expected 446-bp fragment was
revealed after 40 PCR cycles only in IPF samples (lanes 3 and 4). Control lungs did not reveal a positive result, although an equivalent cDNA concentration as analyzed by GADPH amplification was used (Fig. 4, lanes 1 and 2).
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Ki67 and p27 immunostaining and colocalization with TIMP-2
and TIMP-3.
Ki67 and p27 were analyzed in IPF lungs. In general, nuclear p27
staining was more abundant than Ki67 staining, although there were
regional variations in immunoreactivity. Most proliferating cells as
revealed by the presence of the Ki67 antigen were alveolar epithelial
cells and fibroblast-like cells mainly located in areas of fibroblast
foci protruding to the alveolar spaces (Fig.
5A). On the other hand, the
inhibitory cell cycle protein p27 was usually present in most
inflammatory interstitial and intraluminal cells as well as in
endothelial cells (Fig. 5B).
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Collagenase immunolocalization.
Immunoreactive MMP-1 (collagenase-1) was noticed in reactive alveolar
epithelial cells and/or in clusters of alveolar macrophages in all IPF
lungs (Fig. 6A). Besides,
hyperplastic type 2 pneumocytes lining honeycomb cysts in areas of
fibroconnective tissue deposition showed strong staining for MMP-1
(Fig. 6B). Cytokeratin staining corroborated the epithelial
nature of these cells (data not shown). Intriguingly, practically no
interstitial cells producing MMP-1 were noticed.
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Gelatinases A and B and MT-1 MMP immunolocalization.
Regarding type IV collagenases, MMP-2 (gelatinase A) was found in some
foci of subepithelial myofibroblasts (Fig.
7A) located close to areas of
basement membrane disruption. In 8 of 12 of the IPF lungs, MMP-2 was
also observed associated with the ECM surrounding fibroblast foci (Fig.
7B). Normal lungs showed no positive staining (Fig.
7C)
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RT-PCR for fibroblast gelatinase B mRNA.
To corroborate the expression of MMP-9 by lung fibroblasts, we examined
the expression of MMP-9 in cells obtained from normal lungs (~8%
myofibroblasts by -actin staining and fluorescence-activated cell
sorter counting) and in those derived from IPF lungs (40-80% myofibroblasts). Total RNA from nonstimulated and PMA-stimulated fibroblasts was reverse transcribed, and cDNA was amplified as described in MATERIALS AND METHODS. Only fibroblasts
derived from IPF lungs showed a 303-bp fragment amplification that was
increased approximately threefold after PMA treatment (Fig.
9, lanes 3-6). An equivalent cDNA concentration as measured by GADPH amplification with an internal competitor showed no amplification even after PMA
stimulation (Fig. 9, lanes 1 and 2).
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BAL.
Significantly less fluid was recovered from IPF patients (55.4 ± 9.7 vs. 71.3 ± 12.1% in control subjects;
P < 0.01). BAL fluid obtained from IPF patients
revealed a twofold increase in total cell number and exhibited a
significant increase in the percentage of neutrophils and eosinophils
compared with those in the control samples (Table
2).
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SDS-PAGE zymography.
To identify BAL fluid gelatinolytic activities, aliquots adjusted
to 20 µl of lavage fluid were analyzed by gelatin substrate gel
zymography. A representative gelatin zymogram comparing IPF BAL fluid
with that from normal subjects is shown in Fig.
10. BAL normal samples showed faint
bands of 72- and 92-kDa activities corresponding to pro-MMP-2 and
pro-MMP-9, respectively (Fig. 10, lanes N). IPF patients
revealed a marked increase of BAL fluid progelatinase B activity (Fig.
10, lanes 1-4), and in most samples, the
activated form of 86 kDa was also evident. In addition, gelatinolytic bands of higher molecular mass, likely representing
lipocalin-associated progelatinase B specific in neutrophils, were also
noticed. Densitometric analysis showed a 2.5- to 7-fold increase in
progelatinase B activity compared with that in healthy individuals
(Fig. 10). Likewise, IPF BAL fluids displayed a 5- to 15-fold increase
in progelatinase A activity compared with that in control samples. In
the majority of IPF fluids, the 68-kDa active form of pro-MMP-2 was
also observed. All gelatinolytic bands were fully inhibited by EDTA
(data not shown).
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DISCUSSION |
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A dynamic balance between synthesis and degradation of ECM components is required for lung structure and functional maintenance. The loss of regulated turnover may result in a number of different lung diseases including lung emphysema and pulmonary fibrosis.
IPF is characterized by a chronic inflammatory process, with the presence of widely distributed small aggregates of actively proliferating fibroblasts and myofibroblasts, which, in turn, are responsible for the excessive ECM deposition, mainly fibrillar collagens, and alveolar structural remodeling (14). The disease is of a patchy nature, and the progression of the fibrotic lesion until a mature scar at any given time and place reflects an imbalance in ECM synthesis and degradation.
The MMPs, also called matrixins, play a central role in all processes involving ECM remodeling, and an inappropriate regulation of their activities may have pathological implications. Regulation is controlled at several levels including gene transcription and activation of a latent enzyme. Locally, in the extracellular space, MMPs are tightly regulated by TIMPs.
In IPF, the remodeling processes may involve various MMPs and their specific inhibitors, but little is known about their possible participation during lung fibrogenesis.
Our results showed that there are important differences in both localization and abundance of collagenases, gelatinases, and TIMPs in fibrotic tissues. Thus the collagenases MMP-1 and MMP-8, which are responsible for the degradation of interstitial fibrillar collagens, showed a more localized expression compared with TIMPs, and MMP-13, another collagenase, was not found. MMP-1 was usually noticed in alveolar epithelial cells and alveolar macrophages, whereas in the thickened alveolar septa where increased bundles of collagen are accumulating, no positive signal was noticed.
Considering that the main function of collagenases is the removal of fibrillar collagens, the absence in the expression of this enzyme in the interstitium, at least as detected by the methods used in this work, might explain, in part, the presence of scars that do not undergo resorption. Additionally, it has been proposed that MMP-1 expression is induced in primary keratinocytes by contact with native type I collagen and that its degradation initiates keratinocyte migration during reepithelialization (24). In this context, it can be speculated that degradation of basement membrane by upregulated gelatinases in IPF may induce upregulation of collagenase-1 in alveolar epithelial cells, facilitating type 2 cell migration and proliferation (15, 16).
In contrast, TIMP expression was more abundant and usually noticed
associated with the ECM or in interstitium-located cells. Particularly
TIMP-3, which is studied here for the first time in IPF, was copiously
observed throughout the lung parenchyma. This inhibitor was found
exquisitely decorating the elastic lamina in vessels and within the
thickened alveolar septa. Actually, a striking feature of TIMP-3 is
that it is ECM associated, whereas TIMP-1 and TIMP-2 are freely
diffusible extracellular proteins (7). TIMP-3 is not only
important in matrix turnover but also has been shown to induce
apoptosis by the stabilization of tumor necrosis factor- receptors
by an effect dependent on TIMP-3 inhibitory function
(31). Moreover, TIMP-3 overexpression in vascular
smooth muscle cells promoted death by apoptosis by an effect
independent of MMP inhibition (1). Interestingly, it has
been recently demonstrated in mesangial cells that p27, a protein
inhibitor of cell proliferation, may also be involved in apoptosis
(13). Thus it seems that under certain conditions, a
p27-mediated increase in cyclin-dependent kinase-2 activity leads to
apoptosis. In our study, TIMP-3 colocalized with p27 in alveolar
epithelial cells and interstitial inflammatory cells. Apoptosis of type
2 pneumocytes has been demonstrated in vivo in IPF lungs, and it has
been suggested that chronic epithelial cell death may avoid normal
reepithelialization, enhancing the fibrotic response (33).
Several mechanisms may be involved in alveolar epithelial cell
apoptosis, including the Fas-Fas ligand pathway (17) and
fibroblast secretion of apoptotic factors (34), and the
results of the present study suggest the possible participation of
TIMP-3.
TIMP-2 was found almost exclusively associated with fibroblast foci. A fibroblast focus is characterized by a distinct cluster of fibroblasts and/or myofibroblasts within the alveolar wall. The fibroblast foci are distributed throughout the lung parenchyma, representing a characteristic morphological feature in IPF and indicating that fibrosis is actively ongoing (14). These foci may occur in the interstitium as well as in the alveolar spaces (14-16). In the latter, fibroblasts migrate through gaps in the alveolar epithelial basement membranes and proliferate within the alveolar spaces, producing intraluminal fibrosis. This process might be at least partially associated with the secretion of the gelatinases MMP-2 and MMP-9. In this context, both MMP-2 and MMP-9 were observed in subepithelial myofibroblasts and occasionally in areas of denuded alveolar basement membranes, suggesting that these MMPs may play a role in the migration of these cells to the alveolar spaces. As mentioned, subepithelial myofibroblasts were also positive for TIMP-2. Although MMP inhibition is the main function of TIMPs, paradoxically, TIMP-2 might be influencing an enhanced activation of this enzyme through its binding to pro-MMP-2. This feature may be of important physiological significance in modulating the cell surface activation of pro-MMP-2. Such a mechanism should depend on the molar equilibrium between the enzyme and the inhibitor (4). In addition, growing evidence is supporting a wide variety of other functions for TIMPs, including cell growth-promoting activity. In this context, we found that areas of TIMP-2-positive myofibroblasts close to the epithelium showed a positive signal for Ki67, a protein expressed during the cell division cycle in the G1, S, and G2 phases as well as in mitosis.
As previously reported (6, 11), subepithelial myofibroblasts in IPF lungs exhibited immunoreactive MMP-9. Considering that lung fibroblasts do not express MMP-9 in vitro, as we also showed by RT-PCR in cells obtained from human normal lungs, the findings that fibroblasts obtained from IPF lungs expressed the transcript and that expression of gelatinase B was closely related to the percentage of myofibroblasts were of particular importance. Additionally, BAL fluid gelatin zymography showed increased gelatinase activities attributable to MMP-2 and MMP-9 in IPF patients.
TIMP-4 was also explored for first time in IPF lungs. This inhibitor can effectively inhibit human MMPs, and it has been suggested that as TIMP-2, it is more specific for MMP-2. Moreover, it binds to the COOH-terminal domain of MMP-2 in a manner similar to TIMP-2 (12). In normal tissues, TIMP-4 mRNA is confined primarily to the adult heart, and no transcript has been detected in normal lungs (8). In the present study, we demonstrated by RT-PCR, in situ hybridization, and immunohistochemistry that TIMP-4 is highly expressed in IPF lungs, primarily by interstitial macrophages, clusters of plasma cells, and alveolar epithelial cells. Although its role in IPF is largely unknown, the widespread expression found in this study strongly suggests that it may contribute to a profibrotic microenvironment in the IPF lungs.
MT1-MMP has been mainly implicated in the activation of progelatinase A through a trimolecular complex comprising MT1-MMP, MMP-2, and TIMP-2 (3). Intriguingly, by immunohistochemistry, we found that although gelatinase A and TIMP-2 were expressed by the same type of cells, primarily myofibroblasts, MT1-MMP was mainly observed in interstitial cells. Studies are ongoing in our laboratory to analyze the distribution of other MT-MMPs in this disease.
In summary, our findings indicate that during lung fibrogenesis, 1) there is a wider distribution of TIMPs compared with the collagenases MMP-1 and MMP-8 in the lung parenchyma. These findings, together with previous results from our laboratory (18, 23, 28-30) in which we have consistently found a decrease in collagenolytic activity associated with the development of fibrosis, suggest that in IPF a nondegrading fibrillar collagen microenvironment is prevailing; and 2) excessive MMP-2 and MMP-9 production might play a role in basement membrane disruption, enhancing fibroblast invasion to the alveolar spaces.
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ACKNOWLEDGEMENTS |
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We are most grateful to Juan Carlos Valencia for technical photographic support.
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FOOTNOTES |
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This work was supported by Consejo Nacional de Ciencia y Tecnologia (Mexico) Grant CONACYT 27518M and by Programa Universitario de Investigacion en Salud (Universidad Nacional Autónoma de México, Mexico).
Address for reprint requests and other correspondence: A. Pardo, Facultad de Ciencias, U.N.A.M., Apartado Postal 21-630, Coyocán México DF, CP 04000, Mexico (E-mail: aps{at}hp.fciencias.unam.mx).
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. §1734 solely to indicate this fact.
Received 13 January 2000; accepted in final form 20 April 2000.
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