1 Department of Experimental, Environmental Medicine and Biotechnology, University of Milano-Bicocca, Monza 20052; and 2 Department of Animal Biology, University of Pavia, Pavia 27100, Italy
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ABSTRACT |
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We evaluated the changes
in plasma membrane composition, biophysical properties, and morphology
of pulmonary endothelial cells in anesthetized rabbits receiving 0.5 ml · kg1 · min
1 saline
infusion for 180 min, causing mild interstitial edema. Plasma membrane
fractions were obtained from lung homogenates with gradient
centrifugation, allowing a sixfold enrichment in caveolin-1. In
edematous lungs, cholesterol content and phospholipidic phosphorus
increased by 15 and 40%, respectively. These data correlated with
morphometric analysis of lungs fixed in situ by vascular perfusion with
2.5% glutaraldehyde, suggesting a relative increase in surface of
luminal to interstitial front of the capillary endothelial cells, due
to a convoluted luminal profile. In edematous lungs, the fraction of
double-bound fatty acids increased in membrane lipids; moreover, the
phosphatidylcholine/phosphatidylethanolamine and the
cholesterol/phospholipid ratios decreased. These changes were
consistent with the increase in fluorescence anisotropy of plasma
membrane, indicating an increase in its fluidity. Data suggest that
mechanical stimuli elicited by a modest (~4%) increase in
extravascular water cause marked changes in plasma membranes that may
be of relevance in signal transduction and endothelial cell activation.
rabbit; air-blood barrier; endothelial cells; membrane composition and fluidity
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INTRODUCTION |
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THE ALVEOLAR AND CAPILLARY walls delimit the pulmonary interstitium, a thin compartment made of a fiber system, serving as a scaffold, and other macromolecules forming the capillary and the alveolar basement membranes. Extravascular water is distributed within the interstitial compartment of the air-blood barrier and is physiologically kept at a minimum volume to optimize gas diffusion. Recent work, based on an experimental model causing a mild form of pulmonary interstitial edema, allowed us to describe the mechanisms contributing to a tight control of extravascular lung volume in the air-blood barrier (6, 20). These studies also showed that, despite a remarkable resistance of the pulmonary tissue to edema formation, the increase in interstitial fluid volume occurs as a consequence of fragmentation of proteoglycans, important macromolecules of the extracellular matrix (24, 25, 31, 32) controlling microvascular permeability and tissue mechanical resistance. We wished to further investigate the condition of mild interstitial edema because it represents a critical equilibrium between matrix degradation and deposition provided by cellular activation. We focused on cellular involvement in mild interstitial edema, particularly on the composition and fluidity of plasma membranes that are known to be sensitive to alterations in chemical and physical stimuli of the environment surrounding the cells (34, 36).
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MATERIALS AND METHODS |
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Chemicals. The reagents used (analytical grade) and high-performance thin-layer chromatography (HPTLC) plates (Kieselgel 60) were purchased from Merck (Darmstadt, Germany). 3-[Cyclohexylamino]-1 propanesulfonic acid (CAPS), Percoll, calmodulin, NADPH, EDTA, EGTA, phenylmethylsulfonyl fluoride (PMSF), terahydrobiopterin (BH4), and L-arginine were from Sigma Chemical (St. Louis, MO). L-[3H]arginine was obtained from NEN (Boston, MA).
Lung tissue sample preparation for the biochemical analysis of
plasma membranes.
Lung tissue samples were obtained from 10 adult New Zealand White
rabbits (2.53 ± 0.3 kg body wt, mean ± SD) anesthetized with a cocktail of 2.5 ml/kg of 50% (wt/vol) urethane and 40 mg/kg body wt of ketamine injected into an ear vein. Subsequent doses of anesthetic were administered during the experiment, depending on the
arousal of ocular reflexes. Animals were tracheotomized to allow
spontaneous breathing. Samples were obtained from control animals
(killed shortly after anesthesia and tracheotomy; n = 5) and from animals that received slow saline infusion through the
right superior jugular vein (0.5 ml · kg1 · min
1) for 3 h to induce interstitial edema (n = 5). The chest was opened through a midsternal incision (6). Next we opened
the pericardium and cannulated the pulmonary artery by advancing a catheter via the right ventricle. The catheter was secured to the
ventricular wall, and another ligature was placed around the catheter
at the root of the pulmonary artery. An overdose of anesthesia was
given to the animal just before the perfusion. After the left atrium
was sectioned, we perfused the lungs for 3-5 min at room temperature with mammalian Ringer solution (without calcium) containing nitroprusside (20 mg/ml). After this time, the lungs were flushed with
50 ml of 0.25 M sucrose and 20 mM tricine, pH 7.4, with protease inhibitors (solution A) (27). The lungs
were then excised from the chest and immersed in ice-cold
solution A with protease inhibitors. The lung tissue was
then finely minced with a scalpel on a cold glass plate embedded in
packed ice. The minute lung pieces were finally placed in a tube with
30 ml of solution A and homogenized.
Purification of plasma membranes.
Lung homogenates obtained from all control (HC; 5 animals) and
edematous lungs (HE; 5 animals) were subjected to Percoll gradient centrifugation to isolate a plasma membrane fraction (27).
Briefly, the lung tissue was homogenized in buffer (0.25 M sucrose, 1 mM EDTA, 20 mM tricine, pH 7.8), and the lung homogenate was filtered sequentially through 53- and 30-µm filters. Aliquots of filtered tissue homogenates (HC and HE) were then taken for successive analysis,
the remaining part of homogenate was subjected to centrifugation (1,000 g for 10 min) at 4°C, and the supernatant was saved. The resulting pellet was resuspended in 3 ml of buffer and subjected again
to homogenization and centrifugation as above. The two supernatants were combined and overlaid over 25 ml of 30% Percoll in buffer. After
centrifugation using an SW28 rotor at 84,000 g for 45 min at
4°C, we collected a single membranous band readily visible about
Phosphorus analysis and fluorescence spectroscopy. Aliquots of PMC and PME from all animals were used for phospholipid phosphorus determination by the Bartlett (2) procedure. Data were expressed as micromoles per milligrams of protein.
The membrane fluidity of different samples was assessed by fluorescence anisotropy measurements of the fluorescent probe 1,6-diphenyl-1,2,5-hexatriene (DPH) as described (28) with minor modification. A suspension of PMC and PME containing ~200 nmol of phosphorus per 1.5 ml of PBS was used. The fluorescent probe molecule DPH was added to membrane suspension at a final concentration of 10Measurement of nitric oxide synthase activity.
Nitric oxide synthase (NOS) activity was measured in HC and PMC (3 animals) and in HE and PME (3 animals) by monitoring the formation of
L-[3H]citrulline from
L-[3H]arginine (30, 42).
Homogenates (200 µg of protein) and total plasma membranes (50 µg
of protein) were incubated in 150 µl of 50 mM Tris buffer, pH 7.4, containing 0.1 mM EDTA, 0.1 mM EGTA, 1 mM PMSF, 1 mg/ml leupeptin, 2.5 mM CaCl2, 1 mM NADPH, 100 nM calmodulin, 10 µM
BH4, and 5 µM combined L-arginine and
purified L-[3H]arginine (0.5 µC; sp act 54 Ci/mmol) at 37°C for 60 min. The reaction was terminated by
heating samples at 90°C for 10 min. After being cooled,
trichloracetic acid was added to a final concentration of 6% (wt/vol),
and the precipitate was removed by centrifugation (17,000 g,
30 min). One microliter (carrying 6,000 dpm) of the supernatant was
spotted on HPTLC silica gel plates. The HPTLC plates were developed in
the solvent system chloroform:methanol:concentrated ammonia:water
1:9:4:2 (each by vol). Spots for
L-[3H]arginine and
L-[3H]citrulline were quantified with a
-Imager 2000 Instrument (Biospace, Paris, France) using the specific
-Vision software provided by Biospace.
Lipids and fatty acid analysis. Aliquots of HC and PMC (5 animals) and HE and PME (5 animals) were submitted to lipid extraction (40). An organic phase (containing all lipids with the exception of gangliosides) and an aqueous phase (containing gangliosides) were obtained. The lipids were separated on HPTLC plates. The phospholipids from PMC and PME were chromatographed in solution B (chloroform:methanol:acetic acid:water, 60:45:4:2, each by vol). The gangliosides from PMC and PME were chromatographed in solution C (chloroform:methanol:0.2% CaCl2, 50:42:11, each by vol). The cholesterol, from both homogenates and plasma membranes, was chromatographed in solution D (hexane:diethylether:acetic acid, 20:35:1, each by vol). In the case of neutral glycosphingolipids (GLS), the lipids extracted were submitted to alkaline methanolysis (1 h at 37°C in 0.6 N NaOH in methanol) to remove contaminating phospholipids. After extensive dialysis, the GLS were chromatographed in solution E (chloroform:methanol:water, 110:40:6, each by vol). For the analysis of the plasmalogens, the phospholipids were chromatographed in solution B. The plates were then exposed to HCl vapors for 10 min and subsequently chromatographed in solution F for second dimension (chloroform:methanol:acetone:acetic acid:water, 50:15:15:10:5, each by vol). Phospholipids and cholesterol were visualized with anisaldehyde, gangliosides with resorcinol (37), and neutral GLCs with orcinol (39). The plates were scanned with Bio-Rad system and spot identification, and quantification was accomplished by comparison with authentic standard lipids.
Aliquots of different total lipids extracted, corresponding to 100-150 nmol of phosphorus, were submitted to fatty acid analysis (11). Briefly, lipid fatty acids were converted to fatty acid methyl esters in 0.5 N HCl in methanol for 20 h at 80°C. Fatty acid methyl esters were extracted into hexane and analyzed by gas-liquid chromatography (HP-INNOWax capillary column, PEG cross-linked 30 m × 0.32 mm × 0.5 µm; temperature program: 150°C for 1 min, 8°C/min from 150 to 200°C, 2°C/min from 200 to 250°C for 20 min).Lung tissue sample preparation for electron microscopy and
morphometry.
In nine additional rabbits (2.57 ± 0.5 kg body wt, mean ± SD), we performed an ultrastructural morphometric study to evaluate the
changes in cell profile morphology. Lung tissue samples were obtained
from control animals (killed shortly after anesthesia; n = 2), sham animals (kept under anesthesia for 3 h; n = 3), and animals in which interstitial edema was
induced by saline infusion (0.5 ml · kg1 · min
1 for 3 h; n = 4). The animals were anesthetized and
tracheotomized as described above. The pulmonary artery was cannulated
using the surgical approach previously described (6). The
surgical preparation allows the pleural sacs to be left intact,
therefore maintaining the physiological expansion of the lungs.
Perfusion was carried out from two reservoirs arranged in parallel,
connected to the pulmonary artery, and placed at a height of 15 cm
relative to the right atrium that was snipped to allow the drainage of the perfusate. The reservoirs contained saline-dextran (11.06 g NaCl/l,
350 mosM, 3% dextran T-70, and 1,000 units of heparin/100 ml) and the
fixative (phosphate-buffered 2.5% glutaraldehyde with 3% dextran
T-70, total osmolarity 500 mosM, pH 7.4), respectively. An overdose of
anesthesia was given to the animal before the perfusion. The perfusion
circuit was first primed with saline-dextran for ~3 min until the
outflow appeared cleared of blood cells. Fixative was then perfused for
25-30 min. During perfusion, the solutions were added to the
reservoirs to maintain the preset pressure gradient.
Electron microscopy preparation and tissue sampling. In accordance with a stratified random sampling scheme (43), five slices were obtained from the right lungs of control, sham animals, and animals with mild interstitial edema. The stratified random sampling is a suggested scheme to compensate for regional lung differences and to reduce the variability of the sampling means. From each slice, 5-7 small blocks (~1 mm3) were systematically derived and immediately immersed in 2.5% glutaraldehyde for 4 h at 4°C. They were repeatedly washed in 0.1 M phosphate buffer, pH 7.4, postfixed in 1% osmium tetraoxide solution in 0.1 M sodium cacodylate buffer, 3% dextran T-70, and sodium chloride (350 mosM, pH 7.4) for 2 h at 4°C, dehydrated in an ethanol scale, and embedded in Epon 812. Two blocks were randomly selected from each slice and processed for morphometric analysis. The remaining blocks were kept as reserves. Ultrathin sections (600 Å) were cut from the blocks, mounted on uncoated 200-mesh copper grids with uranyl acetate and lead citrate, and examined in a Zeiss EM900 electron microscope. On a single section from each block, seven micrographs of the alveolar parenchyma at ×15,000 magnification were systematically taken and recorded on 70-mm negative films. Thus, sample consisted of 70 micrographs/animal. Morphometric measurements were performed on positive reversal of the negative films.
Morphometric analysis. The volume density (Vv) and surface density (Sv) of alveolar tissue were determined by point and line intersection counting, using established stereological techniques (3, 44). The micrographs at ×15,000 magnification were superimposed with an orthogonal test grid composed of 16 × 16 lines with intersections that yielded 256 test points.
We evaluated the Vv of the extracellular interstitial space and of the cellular compartment (endothelial, epithelial, and interstitial cells) of the alveolar tissue to estimate water distribution in control and edematous lungs. Vv was computed by dividing the number of points falling on each compartment (Pi) by the total number of points falling on the alveolar tissue (Pt): Vv (i,t) = Pi/Pt. To estimate Sv, we counted the number of intersections (I) of the horizontal test lines with the luminal and interstitial boundary profile of endothelial cells and with the alveolar and interstitial boundary profile of epithelial cells. The Sv value was derived in terms of the alveolar tissue volume (t) as: Sv(i,t) = 2 · Ii/(d · Pt), where Ii is the number of intersections per each profile and d is the distance between the test points.Hematocrit and lung weight. A blood sample was taken in control conditions and at the end of the infusion protocol, just before the perfusion procedure, to determine hematocrit. The lungs used for biochemical determinations or electron microscopic morphometry were removed from the chest and weighed. Tissue samples were then taken and weighed fresh and after drying in an oven at 70°C for at least 24 h to determine their wet-to-dry weight ratio.
Statistical analysis. Both biochemical and morphometric data are expressed as means ± SD. Biochemical determinations were repeated three times for each animal. Data from the different animals were averaged. For morphometric analysis, primary data (point and line intersection counts) were summed over all seven micrographs derived from each section, and the parameters (Vv and Sv) were computed as the ratio of sums. The parameters were then averaged over the various section samples. The significance of the differences among groups was determined using one-way ANOVA and Student's t-test.
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RESULTS |
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Comparison of control to edematous lungs. The wet weight of the whole lung was 4.92 ± 0.5 and 4.88 ± 0.4 g/kg body weight in control and edematous animals, respectively. The water content of the lung tissue was estimated from the wet weight to dry weight ratio of lung specimens that averaged 5.3 ± 0.3 and 5.5 ± 0.2 in control and edematous lungs, respectively (4% not significant increase). The dry weight of the lung tissue was estimated by dividing the wet weight by the wet-to-dry weight ratio; it was not significantly different in control and edematous lungs averaging 0.92 ± 0.09 and 0.89 ± 0.08, respectively.
The hematocrit value decreased significantly from 43 ± 2 in control to 36 ± 2 in edematous lungs, reflecting plasma dilution.Morphometric analysis. Cell population of the alveolar septa includes three main cell types: endothelial, epithelial, and interstitial cells (10). Morphological and morphometric analysis was focused on the endothelial and epithelial (alveolar type I) cells in lung parenchyma because they represent the boundary of the alveolar tissue with blood and air, respectively, and therefore display the highest Sv among the cell populations in the septa (7, 13).
Figure 1 shows the ultrastructural appearance of lung parenchyma in control (A) and edematous animals (B). It appears clearly that in control lungs, the endothelium and epithelium are made of thin and smooth cytoplasmic sheets separated by a thin interstitial layer, the three layers together forming the air-blood barrier. In interstitial edema, endothelial cells present an irregular profile with plasma membrane invaginations, mainly on their luminal front. Epithelial cells also show some irregularities on the alveolar front. Note also the enlargement of the basement membranes in edema. The surface irregularities and invaginations of cell profiles on luminal and abluminal sides of endothelial and epithelial cells could be well identified with a magnification of ×15,000.
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Comparison of homogenate to plasma membrane fraction. We determined the content of caveolin-1 that represents a good marker of plasma membrane. We found that it increased about sixfold when comparing homogenate to plasma membrane fraction, thus proving that the purification yielded a satisfactory enrichment.
Measurement of NOS activity.
The activity of NOS (Table 2) was
increased sevenfold when comparing HC to PMC, in line with the expected
enrichment of plasma membrane fraction. It significantly increased
about twofold in PME with respect to PMC.
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Phosphorus analysis and fluorescence spectroscopy. The content of phospholipidic phosphorus in plasma membranes was significantly increased in edematous lungs (Table 2). Using DPH, a fluorescent probe of the membrane fluidity, a significant decrease of the anisotropy parameter r was detected in PME (Table 2), indicating an increase in fluidity.
Lipid analysis.
Aliquots of samples were submitted to lipid extraction, and the
different lipids (cholesterol, ganglioside, neutral glycolipid, and
phospholipid) were separated on HPTLC plates. The cholesterol concentration, normalized to total protein content (Fig.
3), doubled when comparing HC with PMC,
in line with the enrichment procedure. A significant increase in
cholesterol content was observed when comparing PMC with PME. In
control lung plasma membranes, the analysis of gangliosides revealed
that the more abundant ganglioside was GM3 (~45%), followed
by GD1a (17%), GM1 (15%), and GD3 (13%) [ganglioside
nomenclature is according to Svennerholm (38)]. No
changes were found in acid GLS plasma membrane composition when
comparing control with edematous lungs.
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Fatty acid analysis.
Table 3 reports the percentage
composition of total lipid fatty acids from plasma membranes. In
edematous lungs, an increase of linoleic (18:2) and arachidonic (20:4)
acids was found, whereas the palmitic acid (16:0) decreased, leading to
a significant decrease in double-bound index (DBI) from 0.659 ± 0.008 to 0.503 ± 0.01 (P < 0.01).
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DISCUSSION |
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Slow-rate saline infusion leads to mild pulmonary interstitial edema due to an increase in microvascular filtration pressure gradient (due to decreased plasma colloid osmotic pressure) and in filtration area (due to greater lung perfusion). This experimental model has been extensively used in previous work because it offers the advantage to study the sequence of the early events accompanying fluid accumulation in the extravascular space. It was found that the air-blood barrier provides a strong safety factor against the development of severe edema because of its structural resistance. In fact, despite some interstitial matrix damage, it essentially assures low microvascular permeability and low tissue compliance (20). Pulmonary interstitial edema is characterized by a small increase in extravascular water (~4%) and by marked changes in the forces acting on cell surfaces at the interstitial level, due to matrix swelling, and possibly also on the luminal side of endothelial cells, due to variations in shear stress accompanying changes in vascular perfusion.
The present data indicate that mild pulmonary interstitial edema caused marked changes in lipid composition and fluidity of plasma membranes as well as in morphology of endothelial cell profiles. In accordance with our recent work (6), the morphometric analysis did not show differences between sham and control animals, suggesting that the observed changes should depend on the disturbance in interstitial fluid dynamics. Therefore, we were prompted to use only animals killed shortly after anesthesia as control animals for the biochemical analysis.
The purification methods used led to an enrichment of typical plasma membrane components, like caveolin-1, the principal integral protein present in flask-shaped plasmalemma invaginations 50-100 nm in diameter, called caveolae (35). Accordingly, the methods should be considered adequate to study plasma membrane composition. This is also confirmed by the increase of NOS activity and cholesterol content when comparing homogenate to plasma membrane fractions. Concentrations of different plasma membrane components were normalized to total protein content. This appears a valid reference, considering that the dry weight of the lung did not change in interstitial edema.
The increase in plasma membrane fluidity in edematous lungs can be correlated with the decrease of the PC:PE ratio from 1.04 to 0.9, with the cholesterol:phospholipid ratio from 0.22 to 0.185, and also with the decrease of the DBI value from 0.659 to 0.503. These data are in accordance with those obtained in cultured cells and tissues (1, 5, 16, 29). The increase of membrane fluidity can also be explained by a change in fatty acid lipid composition that causes an increase in free volume between the lipid chains, due to the presence of double bounds in fatty acids (18:2 and 20:4), leading to a bend in the lipid chain itself. Plasmalogens have been described to increase with oxidative stress and were also proposed as effective endogenous antioxidants (4). In fact, changes in mechanical stimuli (shear stress) acting on endothelial cells were shown to induce generation of reactive oxygen species (9). Because we found a change in ethanolamine plasmalogen content, we might deduce that mild pulmonary interstitial edema may imply oxidative stress.
The increase in plasma membrane cholesterol and phosphorus content, normalized to total protein, suggests an increase in membrane surface area. The observed changes could be reasonably ascribed to endothelial and epithelial (alveolar type I) cells because they provide most of the surface extension of the air-blood barrier.
An indication of the relative changes in plasma membrane surfaces in interstitial edema may be derived from data in Table 1. The increase in the number of intersections per sample micrograph for the luminal front of endothelial cells as well as the increase in the ratio of the luminal endothelial intersections to the total intersections (luminal + interstitial) indicate that capillary luminal membrane may be relatively increased. The decreased Sv of endothelial and epithelial membranes in edema when referred to alveolar tissue is ascribed to an increase in alveolar tissue volume. This is consistent with a 4% increase in extravascular lung water and the observation that, using the same experimental model (6), a relevant portion (44%) of the extravascular fluid was shown to accumulate in the interstitial compartment of the alveolar septa, causing an ~30% increase in thickness of the air-blood barrier. The latter point is in line with the increase in Vv of the extracellular matrix from 16 to 25% in the alveolar tissue reported in the present study.
More specifically, one can note that the decrease in Sv is larger and significant for the interstitial compared with the luminal endothelial front, in line with a higher surface expansion of the luminal endothelial profile in edema.
The Sv values reported in Fig. 2 are larger than the commonly reported values for the endothelial and epithelial cells that are in the range of 6,000-7,000 cm2/cm3 of alveolar tissue (10, 13). The discrepancy between the present and the reported values could well be accounted for by the difference in sampling procedure and in the final magnification used (7, 13). A high resolution is required to correctly identify surface details.
The increase in plasma membrane phospholipids is likely to reflect an increased synthesis during the experimental study. This would appear consistent with the demonstration that in central nervous system and liver, lipid synthesis is triggered within a relatively short time (33, 41).
The plasma membrane fraction from lung tissue might also include surfactant coming from alveolar surface and from lamellar bodies of alveolar type II cells. The increase in PC (Fig. 5B) that represents an important component of surfactant phospholipids and of caveolae suggests that interstitial edema may cause an increase in vesicle formation and/or in surfactant turnover.
We may attempt to relate biochemical and biophysical changes in plasma
membranes to the changes in physical stimuli acting on endothelial cell
surface. The increase in tissue forces at interstitial level is a
consequence of interstitial fluid accumulation, particularly in the
air-blood barrier as demonstrated by the increased Vv of
the extracellular matrix. Interstitial swelling causes an increase in
interstitial fluid pressure from the physiological value of
approximately 10 cmH2O up to ~5 cmH2O
(20). Because in mild interstitial edema, capillary
pressure remains essentially unchanged at ~10 cmH2O
(21, 23), the above condition should cause a substantial
change in transmural pressure acting across the endothelial cells. In
fact, in physiological conditions, the transmural pressure is
relatively high, averaging 20 cmH2O, the subatmospheric
interstitial pressure pulling on the basal side of the cell. In edema,
on the contrary, the transmural pressure gradient is reduced down to 5 cmH2O, and the positive interstitial pressure pushes on the
basal side of the cell. Furthermore, parenchymal forces exerted at
focal points where cell-matrix attachments occur are expected to
increase as a consequence of swelling of the extracellular matrix.
Morphometry actually revealed only a slight, although not significant,
change in Sv of endothelial cells on the basal side,
reflecting a still regular interstitial profile. This could be
explained by the firm attachment of the cells to the basement membranes
and by the strong structural resistance of the basement membranes in
the air-blood barrier (6).
Furthermore, a change in shear stress could result from the vascular
conditions caused by saline infusion. In a laminar flow regime, shear
stress at the vessel wall () is given by
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Using a fluorescence probe, Haiddekker and coworkers (12) hypothesized that hydrodynamic shear destabilizes the plasma membrane, leading to an increase in fluidity. The membrane alterations could activate membrane-associated signaling proteins, for example heterotrimeric G proteins (15, 19) and endothelial NOS (18, 26). The product of this enzyme, nitric oxide, is a widespread mediator in physiology and functions in the circulatory system as an endogenous vasorelaxant (17). In our experiments, NOS activity doubled in plasma membranes from edematous lungs, suggesting a possible functional relationship to the change in membrane fluidity. Moreover, the increase in NOS activity, in addition to the altered fatty acid profile of plasma membranes [increase of arachidonic acid (20:4)], suggests the activation of transmembrane signaling pathways of the inflammatory process. This is in line with the previous observation demonstrating in mild interstitial edema the activation of metalloprotease-9 of neutrophil origin that cleaves matrix proteoglycans (31, 32).
In summary, although pulmonary interstitial edema implies a modest change in extravascular water, it likely entails mechanical stimuli influencing signal transduction either at cell surface or through the cytoskeleton leading to the release of cytokines and other mediators. Endothelial cells, representing the interface sensing both vascular and parenchymal signals, may be primarily involved to trigger transcription factors and protein expression that in turn influence either matrix deposition and tissue repair or, conversely, activate proteases leading to severe tissue damage.
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ACKNOWLEDGEMENTS |
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The authors thank Prof. G. Bernocchi for useful discussion, Emanuela Clementi for help with preparation of ultrastructural sections, and Dr. Ombretta Bruschi for help with morphometric analysis.
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FOOTNOTES |
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This research was supported by Cofinanziamento, Ministero dell' Università e della Ricerca Scientifica e Tecnologica 1999 (to P. Palestini and G. Miserocchi).
Address for reprint requests and other correspondence: G. Miserocchi, Dipartimento di Medicina Sperimentale, Ambientale e Biotecnologie Mediche, Università di Milano-Bicocca, Via Cadore 48, 20052 Monza (MI), Italy (E-mail: giuseppe.miserocchi{at}unimib.it).
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.
First published February 1, 2002;10.1152/ajplung.00447.2001
Received 20 November 2001; accepted in final form 27 January 2002.
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