Division of Pulmonary and Critical Care Medicine and Will Rogers Institute Pulmonary Research Center, University of Southern California, Keck School of Medicine, Los Angeles, California 90033
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ABSTRACT |
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We
investigated acid-base permeability properties of electrically
resistive monolayers of alveolar epithelial cells (AEC) grown in
primary culture. AEC monolayers were grown on tissue culture-treated
polycarbonate filters. Filters were mounted in a partitioned cuvette
containing two fluid compartments (apical and basolateral) separated by
the adherent monolayer, cells were loaded with the pH-sensitive dye
2',7'-bis(2-carboxyethyl)-5(6)-carboxyfluorescein, and
intracellular pH was determined. Monolayers in
HCO80% by 100 µM
dimethylamiloride, an inhibitor of Na+/H+
exchange, whereas acidification was not affected by a series of
acid/base transport inhibitors. Additional experiments in which AEC
monolayers were grown in the presence of acidic (6.4) or basic (8.0)
medium revealed differential effects on bioelectric properties depending on whether extracellular pH was altered in apical or basolateral fluid compartments bathing the cells. Acid exposure reduced
(and base exposure increased) short-circuit current from the
basolateral side; apical exposure did not affect short-circuit current
in either case. We conclude that AEC monolayers are relatively impermeable to transepithelial acid/base fluxes, primarily because of
impermeability of intercellular junctions and of the apical, rather
than basolateral, cell membrane. The principal basolateral acid exit
pathway observed under these experimental conditions is
Na+/H+ exchange, whereas proton uptake into
cells occurs across the basolateral cell membrane by a different,
undetermined mechanism. These results are consistent with the ability
of the alveolar epithelium to maintain an apical-to-basolateral (air
space-to-blood) pH gradient in situ.
alveolar epithelium; 2',7'-bis(2-carboxyethyl)-5(6)-carboxyfluorescein; 4,4'-diisothiocyanostilbene-2,2'-disulfonic acid; sodium/hydrogen exchange; acidosis
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INTRODUCTION |
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THE ALVEOLAR EPITHELIUM is generally considered to be a tight barrier capable of restricting the movement of salt and water between air space and blood (5, 20). Although most of the daily metabolic acid production passes through it in the form of CO2, little is known about its ability to form a barrier for acid/base equivalents per se. The alveolar space is lined by a thin, continuous layer of fluid [alveolar lining fluid (ALF)], the aqueous subphase pH of which has been measured to be acidic (6.9) relative to blood (7.4) (2, 23). The mechanism by which this gradient is maintained is undetermined, although its existence is presumed to depend primarily on transport and permeability properties of the alveolar epithelium.
The alveolar epithelium has luminal (apical) and serosal (basolateral) aspects functionally compartmentalized by cell-cell junctions. This polarity, which is the structural and functional hallmark of epithelia, makes vectorial transport across the alveolar epithelium possible (13). Apically situated epithelial Na+ channels and basolateral Na+ pumps have been shown to provide the mechanisms for active transepithelial Na+ transport across the alveolar epithelium (5, 20). Other polarized transport mechanisms, including the water channel aquaporin-5 located in the apical membrane of alveolar type I cells (3), are also present in alveolar epithelial cells (AEC). In addition, differences in the composition and functional properties of apical vs. basolateral cell membranes have been shown to exist in epithelia (15, 26), although little is directly known about these differences in AEC.
Several acid/base transport mechanisms have been described in alveolar
epithelium that could contribute to regulation of ALF pH (6, 14,
16-19). These acid/base transport mechanisms, which include
Na+/H+ exchange (NHE1),
Na+-HCO/HCO
The low paracellular permeability of the alveolar epithelium, which is of similar magnitude to other tight epithelia (e.g., toad urinary bladder), is thought to be primarily due to the integrity of the intercellular complexes that link the cells (5). Tight junctions are responsible for maintaining and regulating the paracellular permeability of the alveolar epithelial barrier. The molecular basis by which paracellular permeability is regulated, which probably depends on the expression of specific tight junction proteins that confer relative impermeability to one or more ions, has only recently begun to be understood (11). Although generally assumed to be impermeable to cations, including protons, neither the role of tight junctions in maintaining a transepithelial acid-base gradient across the alveolar epithelium nor the specific junctional proteins involved have been determined.
The goal of the present study is to describe mechanisms whereby the
alveolar epithelium could maintain a transepithelial pH gradient. To
this end, we used a model of the alveolar epithelium in which primary
cultured AEC were grown as electrically resistive monolayers on
permeable supports, permitting independent access to apical and
basolateral aspects of the cells. First, we assessed the ability of
these monolayers to acutely maintain a transepithelial pH gradient.
Second, we studied the differential effects of apical vs. basolateral
changes in pHe on pHi in AEC monolayers. Third, we examined basolateral acid/base entry pathways in AEC. These first
three sets of experiments were performed under CO2- and HCO
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METHODS |
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Preparation of AEC monolayers.
Alveolar type II epithelial cells were isolated from 125- to 150-g male
Sprague-Dawley rat lungs by a modified differential adherence method,
as previously described (8). Briefly, elastase (2-3
U/ml) was used to disaggregate the type II cells from the supporting
lung matrix. The cells were plated on tissue culture-treated Nuclepore
filters (Snapwell; Corning Costar, Acton, MA) at 1.5 × 106 cells/cm2 and maintained in primary culture
in medium consisting of DMEM-Ham's F-12 medium (1:1), BSA (1.25 mg/ml), 10 mM HEPES, 0.1 mM nonessential amino acids, 2.0 mM glutamine,
sodium penicillin G (1,000 U/ml), and streptomycin (1,000 µg/ml). For
experiments in which cells were exposed to altered pHe in
culture (see Effects of extracellular acid and base on AEC
bioelectric properties), cells were cultured in media of identical
composition supplemented with 10% newborn bovine serum and titrated to
pH ~6.0 or ~8.2 using 1 N HCl or KOH for acid or base exposures,
respectively. Transepithelial tissue resistance
(Rt), a measure of monolayer confluence and intercellular junction integrity, and spontaneous potential difference (SPD) across the monolayer were determined daily using a rapid screening device (Millicell-ERS; Millipore, Bedford, MA). Equivalent short-circuit current (ISC), a measure of active
transepithelial ion transport, was calculated from the following
relationship: ISC = SPD/Rt. Experiments are performed 3-4 days
after monolayers were plated, coincident with the development of tissue
resistance 2,000
· cm2, except where
otherwise indicated.
Modified Ussing chamber cuvette for fluorescence measurements. AEC monolayers were mounted in a custom Plexiglas cuvette (California Institute of Technology Machine Shop, Pasadena, CA) designed for fluorescence measurements in a fluorescence spectrophotometer (model LS5B; Perkin-Elmer, Norwalk, CT), as previously described (16-18). The cuvette is diagonally bisected by a Plexiglas slide machined to form a tight seal with the floor and side corners of the cuvette. Before each monolayer was mounted, the filter was detached from its supporting plastic struts. The filter (with the adherent cell monolayer) was then secured in a window in the Plexiglas slide by an O ring, and the slide was positioned in the cuvette. The cuvette is fixed in its position in the spectrofluorometer at 45° to the light source to optimize fluorescence signal from the monolayers. Tissue resistance across the monolayer was determined before and after each experiment using the Millicell screening device by placing the tips of its electrodes on opposite sides of the filter positioned in the cuvette and measuring Rt.
Intracellular loading and fluorescence measurements with a pH-sensitive fluorescent probe. Changes in pHi were monitored using the pH-sensitive fluorescent probe 2',7'-bis(2-carboxyethyl)-5(6)-carboxyfluorescein (BCECF)-AM by methods similar to those used in previous studies (16-18). Briefly, cells were loaded with this lipophilic esterified form of the dye by addition of BCECF-AM to the solution bathing the apical surface of the monolayer from a stock in dimethyl sulfoxide at a 1:1,000 dilution to give a final dye concentration of 15 µM. Loading proceeded in the cuvette at ambient temperature for 30 min.
Previous experiments have confirmed that BCECF is maximally fluorescent in the AEC grown on Nuclepore filters at an emission wavelength of 530 nm and excitation wavelength of 503 nm, with an isosbestic point at 440 nm. Changes in fluorescence intensity were monitored continuously in the fluorescence spectrophotometer at ambient temperature. Cell and filter autofluorescence were noted at 440 and 503 nm before dye loading for each monolayer and subtracted from all fluorescence values when pHi was calculated. Initial change in pHi per unit time (dpHi/dt) was calculated by measuring the slope of a line tangent to the initial deflection of the fluorescence curve. The dpHi/dt was converted to initial H+ flux (JH+) using previously reported values for intrinsic buffer capacity (Calibration of fluorescence vs. pHi. To correlate ratios of fluorescence values at 503- and 440-nm excitation wavelengths to pHi, a calibration curve was constructed at ambient temperature using the K+-nigericin technique (31). AEC monolayers were exposed to BCECF in the presence of buffer containing (in mM) 140 NaCl, 5 KCl, 1 CaCl2, 1 MgCl2, 5 glucose, and 6 HEPES at pH 7.4. After the cells were loaded, the dye-containing buffer was evacuated and replaced by dye-free medium composed of 130 mM KCl, 12 mM NaCl, 1 mM CaCl2, 1 mM MgCl2, 5 mM glucose, 6 mM HEPES, and the K+-H+ ionophore nigericin (1 µg/ml). Because intra- and extracellular K+ concentrations are approximately equal, the nigericin pathway will allow pHi and pHe to become equal. Monolayers are then incubated for 20 min in bathing solutions titrated to a series of different (extracellular) pH values using 1 N KOH or 1 N HCl. In this manner, a series of different pHi values were obtained and the fluorescence ratio was measured. pHi was found to be a linear function of R over the pH range 6.4-8.0, as previously reported (16-18).
Statistical analysis. Values are means ± SE. Significance (P < 0.05) of differences among experimental conditions was determined by ANOVA, except where otherwise indicated.
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RESULTS |
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Impermeability of AEC monolayers to acid and base equivalents.
Monolayers were mounted in the fluorescence chamber and bathed in HEPES
buffer consisting of (in mM) 140 NaCl, 5 KCl, 1 CaCl2, 1 MgCl2, 5 glucose, and 6 HEPES, pH 7.4, in apical and
basolateral fluid compartments. At time 0, fluid in the
basolateral or apical compartments was replaced with fluid of identical
composition at pH 6.4 or 8.0, titrated by addition of HCl or NaOH to
the buffer solution. There was no significant change in pH in either
compartment for any of the four conditions shown in Fig.
1 when fluid was sampled at 30 min, as
determined by t-test (n 3 for each condition). These results indicate that AEC monolayers are relatively impermeable to acid and base equivalents under the conditions of these experiments.
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Apical vs. basolateral membrane permeability to acid and base
equivalents in AEC monolayers.
Representative experiments are illustrated in Fig.
2, in which monolayers were mounted in
the fluorescence chamber, bathed in HEPES buffer at pH 7.4 in apical
and basolateral fluid compartments, and loaded with the fluorescent
pH-sensitive probe BCECF. After a stable baseline was obtained, buffer
in the apical or basolateral fluid compartment was exchanged for buffer
of identical composition of pH 6.4 or 8.0. Replacement of apical fluid
with HEPES buffer at pH 6.4 or 8.0 resulted in minimal changes in
pHi. In contrast, replacement of the basolateral fluid with
HEPES buffer at 6.4 or 8.0 resulted in a significant shift in
pHi in the same direction as pHe. Transmembrane
acid/base fluxes, expressed as dpHi/dt, were
0.08 ± 0.01/min (mean ± SE) for experiments where
basolateral pHe was 6.4 and +0.06 ± 0.01/min for
experiments where basolateral pHe was 8.0 (n
3 for each condition). On the basis of
i for AEC
monolayers, previously reported to be 27 mM/pH unit for
HCO
21.6 and 16.2 mM/min, respectively. These results indicate that the apical membranes of AEC
are relatively impermeable and the basolateral membranes are relatively
permeable to acid or base equivalents.
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Effects of inhibitors on basolateral membrane permeability to
acid/base equivalents in AEC monolayers.
Experiments were performed on AEC monolayers loaded with BCECF as
described above, except 100 µM dimethylamiloride (DMA), 100 µM
DIDS, 100 µM ouabain, 1 mM BaCl2, or 1 mM
ZnCl2 was dissolved in the buffer added to the basolateral
fluid compartment. As illustrated in Fig.
3A (n 3 for each
condition), none of these agents reduced the rate of pHi
decrease due to acid entry when buffer in the basolateral fluid
compartment was exchanged for acidic fluid (pH 6.4). In contrast, DMA
alone inhibited the base equivalent entry step that occurs when
basolateral fluid pH is returned to pH 7.4. As shown in Fig.
3B, DMA similarly blocked the increase in pHi observed when HEPES buffer at pH 8.0 was substituted into the basolateral fluid compartment but did not prevent the fall in pHi observed when pH 7.4 buffer was replaced in the
basolateral fluid. These results suggest that net base entry (or acid
extrusion) occurred at least in part via basolateral
Na+/H+ antiport, whereas net proton uptake
occurred via a different (DMA-insensitive) pathway.
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Effects of extracellular acid and base on AEC bioelectric
properties.
To determine whether prolonged incubation in a transmembrane acid-base
gradient would affect AEC function preferentially via the basolateral
surface, AEC monolayers were incubated in the presence of acidic
(pHe ~ 6.0) or basic (pHe ~ 8.2)
medium on the apical and/or basolateral side of the monolayer from
day 3 in culture, and bioelectric properties were measured
daily thereafter. As indicated in Fig.
4A,
ISC for AEC monolayers grown in apical acidic
medium was not different from that for monolayers grown in pH 7.4 medium, whereas ISC for monolayers grown in
basolateral acidic medium or in acidic medium on both sides was
significantly lower than that for monolayers grown in pH 7.4 medium on
days 4-7. As indicated in Fig. 4B,
ISC for AEC monolayers grown in apical basic
medium was not different from ISC for monolayers grown in pH 7.4 medium, whereas ISC for
monolayers grown in basolateral basic medium or basic medium on both
sides was significantly higher than ISC for
monolayers grown in pH 7.4 medium on days 6 and 7. Differences in ISC
(ISC) between monolayers grown in pH 7.4 medium vs. basolateral acidosis or alkalosis are summarized in Fig.
4C (n
3 for each condition).
Rt was maintained above 2,000
· cm2 through day 5 and was not
significantly different among all conditions (data not shown).
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Effects of adaptation to acidosis and alkalosis on the relationship
between pHi and pHe.
To determine whether prolonged exposure to acidosis or alkalosis
reduced the effects of pHe on pHi via an
adaptive mechanism, AEC monolayers were grown at pH 7.4 for 3 days and
then further cultivated in medium (apical and basolateral) at pH 6.0 (acidosis), 7.4 (control), or 8.0 (alkalosis) for 24 h. AEC
monolayers were then mounted in the cuvette for pHi
measurements (see METHODS) in HEPES buffer at pH 7.4. The
monolayers were subjected to a series of changes in pHe by
exchange of apical and basolateral fluid compartments with HEPES buffer
titrated to pH 6.0-8.0, pHi was allowed to
reequilibrate for ~15 min, and a new steady-state value was recorded.
As illustrated in Fig. 5, control
monolayers responded to changes in pHe with changes in
pHi of similar direction but less magnitude. This
relationship was changed only minimally after 24 h of exposure to
acidic or basic medium, suggesting only limited adaptation in defense
of pHi to extracellular acidosis or alkalosis under the
conditions of these experiments (n 3 for each condition).
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DISCUSSION |
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In this study, we present evidence that AEC monolayers are relatively impermeable to acid/base equivalents under acute and chronic conditions and that they are capable of maintaining an apical-to-basolateral pH gradient in vitro. The ability of these epithelial monolayers to maintain a proton gradient depends primarily on the relative impermeability of the apical membrane and the intercellular junctions to acid/base equivalents. In contrast, basolateral AEC membranes are relatively permeable to net base influx, at least partly via Na+/H+ exchange, as well as acid influx, occurring by another undetermined mechanism. Our results also suggest that intracellular acidosis impairs, and intracellular alkalosis stimulates, active transepithelial Na+ flux, as indicated by the differential effects of apical vs. basolateral exposure on ISC. Finally, we have shown that basolateral pHe substantially affects pHi in AEC monolayers and that this relationship is only minimally affected after 24-48 h of adaptation to altered pHe.
Several lines of evidence indicate that AEC monolayers are impermeable
to acid/base equivalents because of the impermeability of intercellular
junctions and the relative and differential impermeability of the
apical cell membranes compared with the basolateral cell membranes.
First, as shown in Fig. 1, a and b, minimal
transepithelial movement of acid/base equivalents occurs across AEC
monolayers grown on filters when they are incubated in the presence of
a pH gradient for 30 min. Neither the porous polycarbonate filters nor other barriers (e.g., unstirred layer effects) block
acid/base entry at the basolateral membrane (Fig. 2), indicating that
the only impediments to the movement of acid/base equivalents are the
AEC monolayers themselves. Therefore, the intercellular junctions (paracellular pathway) and the cells forming the monolayers
(transcellular pathway) display minimal permeability for acid/base equivalents.
Second, as shown in Fig. 2, exposure of the basolateral surface of AEC monolayers to relatively acidic or basic buffer solutions results in significant changes in pHi. Apical exposure results in minimal change in pHi. Transmembrane movement of acid/base equivalents, across the basolateral membrane itself or via specific membrane transporters, provides the likely explanation for these observed effects. The relative impermeability of the apical membrane correlates with the absence of any acid/base transport mechanisms specifically localized therein and suggests that the relative impermeability of the membrane itself is an adequate explanation for the lack of changes in pHi in the presence of a transapical gradient for pH.
Transmembrane acid/base fluxes occur across the basolateral membranes
of AEC, at least in part via membrane transporters. As shown in Fig. 3,
intracellular alkalinization due to the presence of a transmembrane
gradient across the basolateral membrane (pHe > pHi) is reduced when DMA is present in basolateral fluid.
These results suggest that pHi is increased by acid exit
(or base entry) via the Na+/H+ exchanger
(NHE1), previously shown to be present on the basolateral membrane of
these cells (17). Acid efflux (i.e., base
loading) is characteristic of Na+/H+ exchange
in AEC, although reversal of Na+/H+ exchange
resulting in net acid influx is also possible in the presence of a
large outwardly directed gradient for Na+ across the
basolateral membrane (17). Nonetheless, acid entry across
the basolateral membrane occurs by a mechanism that is not inhibitable
by DMA or by a panel of inhibitors of other potential acid entry
pathways. DIDS, an inhibitor of HCO/HCO
/OH
and
Cl
/base exchange) are also not present or do not
contribute to acid influx (10, 27). Despite literature
suggesting that other transporters such as Na+ pumps and
channels, K+ channels, and H+ channels could
provide an entry pathway for acid equivalents in these or other cells
(6, 7, 12, 32), their respective inhibitors or blockers
(e.g., ouabain, BaCl2, and ZnCl2)
also had no effects. Taken together, these results are consistent with proton permeability directly across the basolateral membrane or, more
likely, net acid efflux primarily via Na+/H+
exchange and acid influx via some other as yet undetermined
mechanism(s) in the presence of an acid-base gradient.
A third line of evidence for the differential permeability of apical and basolateral membranes of AEC to acid/base equivalents and the ability of their intercellular junctions to prevent transepithelial acid/base fluxes comes from experiments performed on cells maintained in media of various pH. Electrically resistive AEC monolayers maintained in media titrated to acidic or alkaline pH facing apical or basolateral sides of the monolayer on days 4-7 in culture show no significant loss of the pH gradient for the entire time they are maintained in this fashion (data not shown). Nonetheless, cells grown in the presence of a basolateral transmembrane gradient for pH develop changes in bioelectric properties that are not evident in the presence of an apical gradient. As shown in Fig. 4, A and C, ISC (a measure of active transepithelial Na+ transport) across AEC monolayers is reduced within 24 h in the presence of basolateral acid (or apical and basolateral acid) relative to cells exposed only to apical acid (or no pH gradient). As also indicated in Fig. 4, B and C, ISC is increased in the presence of basolateral (or basolateral and apical) alkalinity relative to cells exposed only to apical base (or no pH gradient). In neither case did exposure of the cells on days 4-7 to acid or alkaline medium significantly change Rt (a measure of monolayer confluence or integrity of intercellular junctions; data not shown), consistent with the ability of the AEC monolayers to maintain a pH gradient (and to transport Na+ in a vectorial fashion) over several days in culture.
Direct effects of pHe on basolateral membrane active transport properties (e.g., Na+ pump activity) and ISC cannot be completely separated from effects mediated via changes in pHi on the basis of our results. The permeability of the basolateral membranes of AEC to acid/base equivalents makes it difficult to distinguish effects of pHi from pHe. pHi in AEC cannot be chronically changed by exposure to altered pHe, as described here if basolateral medium is restored to pHe 7.4, for example, in the absence of a specific inhibitor of acid entry via the basolateral membrane (Fig. 3). Further distinction between the effects of intra- and extracellular acidosis will therefore require a method, presently unavailable, of chronically acidifying and alkalinizing AEC while the membranes are maintained in a pH 7.4 medium.
Interpretation of experiments where medium pH was changed at the apical membrane (where changes in ISC were not observed and alterations in pHi were not anticipated) is somewhat more straightforward. The lack of effect of chronic changes in apical medium pH on ISC indicates that active transport is not altered by changes in pHe at the apical membrane and is further compatible with a lack of effect of pHe on pHi via apical acid/base transport. Taken together, the results illustrated in Fig. 4 are most consistent with the concept that chronic changes in pHi result from basolateral (but not apical) acid/base transport. Furthermore, although direct effects of pHe on basolateral membrane active transport properties cannot be excluded, it appears likely that at least some of the observed effects of basolateral pHe are mediated via changes in pHi.
Although the cellular mechanisms by which changes in pHi
(and/or pHe) alter transepithelial transport in AEC cannot
be determined at this time, several possibilities exist. The
permeability of epithelial Na+ channels (ENaC) and activity
of Na+ pumps are potentially altered by pH changes
(4, 29), with direct changes occurring over a short time
course (i.e., minutes). The observed changes in
ISC in the presence of basolateral pH gradients
occurred over a time course of several hours (data not shown),
suggesting that an indirect mechanism (e.g., change in cellular ATP levels) could be responsible. Alternatively, a change in
gene expression or protein turnover of one or more Na+
transporters could have contributed to the observed changes in ISC. Measurements of steady-state levels of
Na+ pump -subunits by immunoblot (data not shown) showed
no change in the presence of an increase or decrease in
ISC induced by basolateral alkalosis or
acidosis, however, suggesting that other mechanism(s) are operative.
Whatever the mechanism of altered Na+ transport in the presence of a basolateral proton gradient, it appears very likely that differential effects on pHi occur in chronic experiments in a manner similar to those that occur acutely (Figs. 2 and 3). Because the pHi of AEC monolayers could not be measured directly while monolayers were being cultivated in 5% CO2 over several days and given the known ability of several different kidney cell lines to adapt to changes in pHe by changing transporter activity and/or intracellular buffer capacity (24, 30), experiments were performed after 24 h of incubation in the presence of acidic or alkaline medium to determine whether adaptation occurs that could limit pH changes in chronically exposed cells. Monolayers were subjected to a series of different pHe buffers (apical and basolateral), pHi was determined, and, as indicated in Fig. 5, little difference in the response of pHi to pHe was observed. These data suggest that minimal adaptation occurred over 24 h of culture in the presence of altered pHe. Whereas it is possible, perhaps likely, that such adaptation could occur over longer periods of time to protect cells from the effects of, for example, prolonged acidosis, the absence of significant adaptation is consistent with the development of changes in pHi with chronic experimental exposure to basolateral (but not apical) pH gradients similar to those found acutely.
Taken together, these data indicate that AEC monolayers restrict the movement of acid/base equivalents because of the impermeability of the apical membrane of AEC and the intercellular junctions between them to protons (or their equivalent). The apparent lack of specific acid/base permeability pathways (i.e., channels, carriers, or transporters) active at the apical membrane and the impermeability of the apical membrane itself to acid/base equivalents are probably sufficient to explain the results of acute and chronic experiments showing a lack of effect of apical pH gradients on pHi or ISC, respectively. In contrast, there is insufficient information at this time to fully explain the mechanisms by which intercellular junctions restrict acid/base movement across AEC monolayers. These effects most likely result from specific properties of the tight junctions present in these electrically resistive monolayers (11).
One implication of these results is that pHi of AEC may be more closely related to plasma or interstitial pH than to alveolar pH. This was first proposed in 1969 by Effros and Chinard (9) on the basis of a study in which they estimated the extravascular pH of the lung in dogs by measuring the pH-sensitive distribution of nicotine across the pulmonary vasculature. Changes in pulmonary extravascular pH occurred more closely in parallel to changes in arterial pH than to alterations in PCO2 at constant arterial pH. These findings led the authors to suggest that relative insensitivity of tissue pH to changes in PCO2 at constant plasma pH could be advantageous in the lung, which is exposed to rapid variations in PCO2. The authors further concluded that the stability of pulmonary tissue pH could be linked to blood (and thereby whole body) acid-base balance, rather than to local buffering mechanisms alone, the latter being particularly vulnerable to changes in alveolar ventilation. Although our present findings do not specifically address the issue of the role of PCO2 in regulation of alveolar epithelial cell pHi, they are consistent with the concept that these cells are sensitive to changes in basolateral (i.e., plasma or interstitial), rather than apical (i.e., alveolar), pH in a fashion similar to that described in situ by these authors.
Our present results are not consistent with the hypothesis of DeCoursey
(7), in which a role for proton channels in the excretion
of CO2 by the lung has been proposed. In a recent review on
the subject (7), the author suggested the possibility that CO2 could be at least partly excreted across the apical
membrane of AEC as H+ and HCO
In summary, we have shown that AEC monolayers grown in primary culture on polycarbonate filters are relatively impermeable to acid/base equivalents because of the impermeability of the apical membrane of the AEC and the intercellular junctions between them. The basolateral membranes of AEC are freely permeable to acid/base equivalents that enter and exit the cells via one or more known basolateral acid/base transporters in addition to other as yet undetermined mechanisms. Chronic exposure of AEC monolayers to basolateral (but not apical) pH gradients results in changes in transepithelial Na+ transport likely due to changes in pHi that appear not to be blunted by intracellular adaptation to acidosis or alkalosis. These results suggest that acid/base impermeability is a fundamental property of the alveolar epithelium and are consistent with the ability of the alveolar epithelium to maintain an air space-to-blood pH gradient as observed in situ. They also suggest that chronic changes in systemic pH, as occur in chronic metabolic acidosis, could affect the ability of the alveolar epithelium to transport Na+ for maintenance of alveolar fluid balance and resolution of alveolar edema.
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ACKNOWLEDGEMENTS |
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We appreciate the expert technical support of M. J. Foster, S. Parra, and J.-R. Alvarez. We also thank L. Lamb (California Institute of Technology) for invaluable assistance in the production of the cuvette.
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FOOTNOTES |
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This work was supported in part by the American Lung Association, the American Heart Association-Western States Affiliate, National Heart, Lung, and Blood Institute Research Grants HL-03609, HL-38578, HL-38621, and HL-51928, and the Hastings Foundation. E. D. Crandall is Norris Chair and Hastings Professor of Medicine.
Address for reprint requests and other correspondence: R. L. Lubman, University of Southern California, Keck School of Medicine, HMR 900, 2011 Zonal Ave., Los Angeles, CA 90089-0110 (E-mail: rlubman{at}hsc.usc.edu).
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.
10.1152/ajplung.00330.2001
Received 15 August 2001; accepted in final form 1 November 2001.
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