Dept. Fisiología y Biología Animal, Facultad de Farmacia, Universidad de Sevilla, 41012 Sevilla, Spain
Received on June 3, 2003; revised on October 1, 2003; accepted on January 11, 2004
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Abstract |
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Key words: D-mannose / enterocytes / intestine
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Introduction |
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Early studies using epithelial cells revealed that rodent small intestine absorbed D-mannose at a rate lower than that of glucose (Cori, 1925; Deuel et al., 1938
; Wilson and Vincent, 1955
). Alton et al. (1997)
observed in rats that following a gavage dose containing 3H-mannose, nearly all of the radioactivity first appearing in the blood was 3H-D-mannose, rather than 3HOH, and that less than 1% of total 3H-mannose was in either feces or intestinal contents. They concluded that D-mannose crosses the enterocytes very efficiently. These studies, however, did not address the mechanisms that mediate transepithelial D-mannose transport.
The transepithelial transport of D-mannose requires transporters located at the apical and basolateral membrane of the epithelial cells. An apical Na+-dependent D-mannose transport system has been described in flounder (Pritchard et al., 1982), dog (Mendelssohn and Silverman, 1989
; Silverman and Ho, 1993
), and rat (Blasco et al., 2000
; De la Horra et al., 2001
) kidney; in LLC-PK1 cells (Saito et al., 1996
); in Caco-2 cells (Ogier-Denis et al., 1994
); and in chicken (Cano et al., 2001
) and rat (De la Horra et al., 2001
) small intestine. This Na+/D-mannose transport system is saturable, is electrogenic, and has a substrate specificity and kinetic properties different from those of SGLT-1 transporter. Ogier-Denis et al. (1994)
also described the presence of a Na+-independent D-mannose transport system in the basolateral membrane of Caco-2 cells.
The mannose concentration in the mammalian intestinal lumen, ready to use the Na+/D-mannose cotransporter, is unknown because data on the content and bioavailibity of mannose in the foods and on intestinal glycoproteins digestion are not available. However, the identification of -mannosidase I and II on the enterocytes brush border (Velasco et al., 1993
) suggests that they could function in glycoprotein digestion and therefore provide mannose to the apical Na+/D-mannose transporter.
The current study was designed to further investigate intestinal D-mannose transport. Avian enterocytes were preferred to those from mammals, because, at least in our hands, the rat enterocyte preparations give very low yields and do not remain alive for more than 15 min. In addition previous studies revealed the presence of Na+/mannose cotransport activity in both, chicken (Cano et al., 2001) and rat (De la Horra et al., 2001
) small intestine.
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Results |
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The data shown in Figure 1A represent total soluble cell [3H]-substrate. However, under either Na+-free or ice-bath conditions, soluble label [3H] cell content was higher than that in the external medium, indicating that part of the [3H]-sugar it is not in a readily diffusible form. In some experiments cell pellets were extracted with barium/zinc to precipitate phosphorylated sugar (Somogy, 1945). Also, the amount of label converted to 3H2O during its entry into glycolysis was estimated as described in Materials and methods and subtracted from the total soluble label. After these corrections were done, the inside:outside sugar ratio is 1:1 in Na+-free conditions (Figure 1B), and the transference of those cells, which have been transporting mannose in the presence of Na+, to ice bath releases the previously taken mannose until the intra- to extracellular mannose concentration ratio was 1 (Figure 1B). These observations indicate that part of the mannose taken up by the enterocytes is phosphorylated and converted to water.
Identification of enterocyte radioactivity
Experiments were carried out to further determine what proportion of D-mannose taken by the cells remains either as free mannose, is converted to H2O, is phosphorylated, or is bound to membrane components.
To evaluate the D-[2-3H]-mannose associated to membrane components (glycoproteins), cells were precipitated by perchloric acid (PCA) and the radioactivity present in the supernatant (free mannose, phosphorylated sugar, and 3H2O) and that in the pellet (bound to membranes) was measured. As mentioned, extraction with barium/zinc was used to evaluate the sugar-phosphate content. Label conversion to 3H2O was evaluated as described in Materials and methods. To evaluate total mannose uptake (free plus phosphorylated plus bound to cell membranes plus metabolized to water), the enterocytes were separated from the incubation buffer by a rapid filtration technique (De la Horra et al., 2001), and the filters containing the cells were placed in the scintillation fluid.
The results (Figure 2) reveal that after 5 min incubation 40% of the total mannose taken by the cells is incorporated into membrane components, and this amount increases with time. In all the times tested the phosphorylated sugar represents
7% of the total label taken by the cells, that is, 12% of the total radioactivity present in the supernatant. At 5 min the free mannose represents 36% of the total taken up by the cells, and it decreased to 25% at 60 min. The amount of label that corresponds to 3H2O represents a 16%, 13%, and 11% of the total label present in the cells at 5, 15, and 60 min, respectively, or 30% of label present in the cell lysate. Altogether these results indicate that part of the mannose taken up by the cells is rapidly metabolized.
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Specificity of D-mannose transport
D-mannose and 3-O-methyl-glucose (3-OMG) uptakes were measured in the absence and presence of the compounds listed in Table I. The results show that D-mannose uptake was nearly abolished by unlabeled D-mannose (97% inhibition), inhibited by -methyl-glucopyranoside (44% inhibition) and phlorizin (40% inhibition), and unaffected by D-fructose. The phlorizine-insensitive mannose uptake was nearly abolished by D-mannose but not by
-methyl-glucopyranoside.
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Effect of phloretin and cytochalasin B on the steady-state sugar cell concentration
Glut2 mediates glucose efflux from the enterocytes. This transporter is Na+-independent and phloretin- and cytochalasin Bsensitive. Figure 4 reveals that, as shown by Kimmich and Randles (1975), addition of either phloretin or cytochalasin B at the steady-state 3-OMG cell accumulation induced a transition to a new steady state, in which a higher cellular 3-OMG concentration is maintained because its basolateral efflux is prevented. However, phloretin or cytochalasin B reduced cell mannose concentration (Figure 4).
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Discussion |
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However, at a difference from membrane vesicles, intact cells provide information regarding the fate of the mannose taken up by the apical membrane transporter. The current results revealed that under either Na+-free or ice-bath conditions mannose concentration within the cells was higher than in the external medium, suggesting that once in the cells part of the mannose is converted into a nonreadily diffusible form. Chromatographic studies and radioisotope measurements revealed that part of the mannose taken up by the cells is either bound to cell membranes, phosphorylated, or converted to 3H2O, and the rest remains as free mannose. Whereas the amount of phosphorylated sugar remains relatively constant, that bound to cell membranes increased and that remaining as free mannose decreased with time. Additionally, the percentage of label that corresponds to 3H2O decreases from 16% at 5 min to 11% at 60 min.
These findings indicate that part of the mannose taken up by the enterocytes remains as free mannose, ready to cross the basolateral membrane toward the blood. Therefore, mannose somehow escapes enterocyte metabolism, a conclusion that can also been reached by comparing enterocyte PMI activity and mannose transport values. Thus the measured PMI activity (10 nmol/min/mg protein) is at least 10,000 times higher than total mannose uptake (around 0.5 pmol/min/mg protein). How can mannose remain free in the cytosol? One could speculate that mannose and PMI are in separate cell compartments. Contrary to the current observations, Panneerselvam et al. (1997) found that human fibroblasts convert 8590% of the transported mannose into water. However, at a difference from fibroblasts, enterocytes are designed to undergo net transepithelial transport of substrates.
Previous reports agree with the aforementioned point of view. Thus, Alton et al. (1997, 1998
) observed that 8 h after a gavage dose of [2-3H]mannose, only less than 1% of total label was found in rat feces and intestinal contents, indicating that intestinal absorption of mannose was highly efficient. They also concluded that mannose transcytose the enterocytes because nearly all the radioactivity first appearing in the blood was found as [2-3H]mannose rather than as 3H2O. Additionally, oral mannose intake leads to an increase in blood mannose levels (Davis and Freeze, 2001
; Westphal et al., 2001
).
Since the molecular characterization of the first facilitative-diffusion glucose transporter (GLUT1), 12 other hexose transporters have been identified: GLUT2 to GLUT12 and the proton-myoinositol symporter (Joost et al., 2002). Of these 13 transporters, GLUT2 and GLUT5 are expressed in the enterocyte basolateral and apical membranes, respectively (see Thorens, 1996
for review; Rogers et al., 2001). Very low amounts mRNA GLUT8 have also been detected in small intestine (Doege et al., 2000
; Ibberson et al., 2000
). The tissue distribution and hexose expecificity of GLUT12 is so far unknown. The following observations suggest that neither GLUT1, GLUT2, GLUT5, nor GLUT8 mediate mannose efflux from enterocytes. Thus the GLUT1 and GLUT2 inhibitor phloretin reduced D-mannose cell concentration and did not affect mannose efflux rate; however, it enhanced the steady-state Na+-dependent gradient of 3-OMG and inhibited glucose efflux rate. Furthermore, fructose, the GLUT5 substrate (Burant et al., 1992
) also transported by GLUT8 (Ibberson et al., 2000
), does not affect mannose efflux rate. The current results do not agree with those previously reported in differentiated Caco-2 cells (Ogier-Denis et al., 1994
), wherein phloretin and fructose highly inhibited the basolateral membrane Na+-independent mannose uptake.
In conclusion, enterocytes transport mannose, and 5167% of the mannose taken up by the cells is metabolized. For mannose transport, enterocytes present at least two D-mannose-specific carrier-mediated transport systems. One is concentrative, Na+- and voltage-dependent, and located at the apical membrane. In contrast, D-mannose efflux from the enterocytes resembles a facilitated diffusion process that is mediated by a phloretin- and cytochalasin Binsensitive and Na+-independent transport system. The current results offer no clue on the nature and cellular location of the Na+-independent D-mannose transport system(s). Locus of the Na+-independent transport system is tentatively ascribed to the serosal cell surface, where it would serve for mannose transfer between enterocyte and lamina propia of the villus.
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Materials and methods |
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Reagents and solutions
Unless otherwise stated the incubation buffer contained, in mM: 100 NaCl, 1 CaCl2, 70 mannitol, 3 K2PO4, 1 MgCl2, 20 HEPES-Tris, pH 7.4, and 1 mg/ml bovine serum albumin. One millimolar L-glutamine was present in all the solutions as passively transported nutrient. The uptake buffer also contained either 0.2 µM D-mannose with tracers of D-[2-3H]-mannose. When used, the concentration [14C]-3-OMG was 1 µM.
Animals, cell isolation, and D-mannose uptake measurements
The experiments were performed in accordance with national/local ethical guidelines. Hubbard chickens, 46 weeks old, were killed by decapitation. Enterocytes were isolated by hyaluronidase incubation as described by Calonge et al. (1989) and incubated at 37°C, under the desired experimental condition. Uptake was terminated by diluting 200 µl cell suspension in 800 µl ice-cold buffer, and the cells were separated by centrifugation through a layer of an oil mixture (Calonge et al., 1989
). Cell pellets were extracted with either 3% PCA or with Ba(OH)2 and ZnSO4 (barium/zinc). Aliquots (100 µl) of the supernatants were added to vials for scintillation counting. D-mannose uptake was calculated taking into account the trapped extracellular volume and cell water volume, as previously estimated (Calonge et al., 1989
). The pellet protein was measured by the method of Bradford (1976)
.
Chromatographic identification of cell-free D-mannose and phosphorylated monosaccharides
The enterocytes were incubated with D-[2-3H]-mannose and treated as described, except that the cell pellets were extracted with ethanol:water (1:1). Aliquots of the extract were spotted on silica gel thin-layer chromatographic plates along with 2 µg nonradioactive D-mannose and 5 µg mannose-6-P. Ascending chromatography was performed on the plates using a solvent system consisting of (v/v), 20 benthene:20 acetic acid:60 methanol. The lanes, to which radioactivity was applied, were cut into 1-cm sections. Each section was placed in scintillation vial and counted. The remaining portion of the plate, which contained nonradioactive D-mannose and mannose-6-P standards, was visualized with anisaldehyde sulfuric acid. The relative mobilities were calculated from the visualized spots and from radioactivity measurements.
Quantification of glycoprotein-associated [2-3H]-mannose
Radioactivity incorporated into glycoproteins was determined by adding an equal volume of 3% PCA to an aliquot of cells. After vortexing and standing 10 min on ice bath, the precipitated protein was collected by centrifugation. The pellet was washed twice with 3% PCA and resuspended in protosol (Dupont, Boston) for radioactivity counting.
PMI assays
PMI activity was measured as described by Davis and Freeze (2000) in both rat and chicken enterocytes. Briefly, PMI was obtained by homogenization of isolated enterocytes in 50 mM HEPES (pH 7.1) and collecting the supernatant from a 100,000 x g centrifugation (1 h). PMI activity assay was carried out in 50 mM HEPES (pH 7.1) containing 50 µg protein, 5 mg MgCl2, 0.25 Nicotinamide adenine dinucleotide phosphate (NADP), and 0.5 U/ml each of phosphoglucoisomerase and glucose 6-phosphate dehydrogenase. The reaction was initiated by addition of 1 µmol/ml D-mannose-6-phosphate. The samples were incubated at room temperature and the optical density at 340 nm was measured.
3H2O Determination
At the end of the experiment, aliquots from either the incubation medium or the cell lysate were evaporated to dryness, suspended in water, and counted. The amount of 3H2O formed was taken as the difference between the initial amount of radioactivity in either the incubation medium or cell lysate and that remaining after evaporation. Both methods provide similar results.
Sugar efflux measurements
Enterocytes were loaded by incubation with either 0.2 µM D-[2-3H]-mannose or 1 µM 3-[14C]-OMG in a shaking water bath at 37°C for 30 min. The cells were then washed twice in radioisotope-free ice-cold buffer and resuspended in the desired buffer. The rate of sugar loss from the cells was measured by diluting 0.5 ml of the sugar-loaded cell suspension into 2.5 ml of radioisotope-free buffer kept at 37°C. Aliquots of 200 µl were taken at 0, 2, 4, and 8 min, and the radiolabeled sugar in the cell pellet was measured as indicated. Sugar efflux was evaluated as percent of radiolabeled sugar remaining in the cells and expressed as an apparent efflux rate coefficient that has the units of min1.
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Acknowledgements |
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Footnotes |
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Abbreviations |
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References |
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