text new page (beta)
English (pdf)
Article in xml format
Curriculum ScienTI
Automatic translation
Cited by SciELO 
Cited by Google 
Similars in
SciELO 
Similars in Google 
uBio 
Permalink
INTRODUCTION
Diabetes mellitus is a heterogeneous clinical syndrome characterized by endocrine-metabolic abnormalities that alter homeostasis. The neurological manifestations are probably the most common among the chronic complications caused by diabetesmellitus. Diabetic neuropathy is a heterogeneous group of disorders, with an extensive range of abnormalities (Vinik and Mehrabyan 2004), that can affect the peripheral nervous system harming the quality of life of individuals (Vinik 1999, Afzaal and Saleem 2002).
Many studies have demonstrated alterations in the myenteric plexus of several intestinal segments of diabetic rats, not just regarding the reduction on the number, but also on the size of neurons (Belai et al. 1988, 1991, Belai and Burnstock 1990, Zanoni et al. 1997, 2003). An important factor related to the diabetic neuropathy is oxidative stress (Vinson et al. 1989, Baynes 1991), which happens when there is an increase of reactive oxygen species (ROS) (Parthiban et al. 1995, Kuyvenhoven and Meinders 1999) and/or a reduction on the efficiency of the endogenous antioxidants (Baynes 1991, Kuyvenhoven and Meinders 1999).
Another factor that provokes neuronal degeneration is the intracellular increase of sorbitol and fructose, due to the increase of the aldose reductase enzyme activity in the polyol metabolic pathway as a consequence of hyperglycemia (Vinik 1999, Giugliano et al. 1996, Afzaal and Saleem 2002). As the glucose conversion by aldose reductase into sorbitol consumes NADPH, there is a reduction on the ratio NADPH:NADP+ (Giugliano et al. 1996). That reduction can impair the reactions that NADPH need, especially the oxidized glutathione conversion to reduced glutathione by the glutathione reductase. Consequently, reduced levels of glutathione is observed in diabetesmellitus, which increases the susceptibility of cells to oxidative stress (Vincent et al. 2004). Hence, measures that increase the availability of antioxidants may be relevant in the treatment of the chronic complications associated with diabetes mellitus. Within this context, the L-glutamine supplementation is likely to present some neuroprotective effects, since it is a substrate for the production of glutathione (Amores-Sánchez and Medina 1999).
L-glutamine is a non essential amino acid, stored mainly in the skeletal muscle (75%) and in the liver (25%). Among its multiple functions, L-glutamine serves as primary carrier of nitrogen among the tissues and it is the main source of energy for the speed proliferation of cells, such as the intestinal epithelium (Vahdat 2001). L-glutamine is metabolized through the phosphate-L-glutaminase, resulting in glutamate and ammonia. Glutamate is transported to the cytosol and it can be used in the synthesis of glutathione (Amores-Sánches and Medina 1999), thus, maintaining the glutathione concentration in the cells. The absence of L-glutamine compromises nitrogen transport, causes a depletion of energy and a reduction on the glutathione levels (Wolfgand et al. 2003). According to Watford et al. (1984), there is a reduction of the plasmatic L-glutamine during diabetes mellitus. Therefore, it is possible that glutamine may help to keep the integrity of the intestinal mucosa in diabetes mellitus.
The objective of this work was to evaluate the effect of the L-glutamine supplementation on myosin-V-stained myenteric neurons and on the mucosa in the ileum of streptozotocin-induced diabetic rats.
MATERIALS AND METHODS
Procedure with the Animals
All of the experiments described in this work were supervised and approved by the Committee of Ethics on Animal Experimentation of the Universidade Estadual de Maringá. Twenty-five male Wistar rats (Rattus norvegicus), 90 days of age were used. Diabetes was induced through the intravenous administration of 35 mg.kg−1 of body weight of streptozotocin (Sigma, St. Louis, USA), dissolved in a buffer solution of 10 mmol.L−1 (pH 4.5), prior to a 14-hour-fast. The injection with streptozotocin resulted in the diabetic syndrome with polyuria, polyphagia and polydipsia. The glycaemia (Bergmeyer and Bernet 1974) of each animal was assessed on the 4th day after the diabetes onset, with a mean value of 486.9 ± 14.25 mg.dL−1. The rats were divided in five groups: untreated normoglycaemic (UN), normoglycaemic treated with L-glutamine (NG), untreated diabetics (UD), diabetics treated with L-glutamine, starting on the 4th (DG4) or 45thday following the onset of diabetes (DG45). The amount of food intake, water consumption and eliminated urine were assessed for five days of the last week of every month, with use of metabolic cages.
The animals were kept in individual cages, receiving water and food (Nuvital® lab) ad libitum, with a photoperiod (6 am - 6 pm) and controlled room temperature (24°C±2°C). Some animals were fed chow supplemented with L-glutamine (1%) (Ajinomoto, Tokyo, Japan), which was prepared weekly.
On the 210th day, the animals were anesthetized with sodium thiopental (40 mg.kg−1 of body weight) and their blood collected by heart puncture to measure the glucose (Bergmeyer and Bernet 1974).
Neuronal Counting and Morphometric Analysis of Myenteric Neurons
The rats were perfused with 250 mL of fixing solution containing sodium periodate (10 mM), lysine (75 mM), paraformaldehyde (1%) in phosphate buffer (PB), pH 7.4 (37 mM) followed by a 1.1% saline solution. After perfusion, each ileum was removed, rinsed with saline solution, opened and immersed for 1 hour in the same fixing solution. Subsequently, the segments were dehydrated in ethanol (50, 70, 80, 90, and 100%), remaining in each solution for 10 min, cleared in xylol (10 min), rehydrated with 100, 95, 90, 80, 70% ethanol, and stored in 70% ethanol. Afterwards, the segments were dissected under a stereomicroscope with transillumination, to remove the mucous and submucous layer, obtaining whole mount external muscle layers preparations. The neurons were stained for immunoreactivity to myosin V (Drengk et al. 2000) as described previously using an antibody developed in the laboratories of Cellular and Molecular Biology Department, Universidade de São Paulo (USP), Ribeirão Preto. These preparations were rinsed twice in phosphate-buffered saline (PBS) 0.1 M, pH 7.4 and blocked with PBS, bovine serum albumin (BSA) (2%) (Sigma, St Louis, MO, USA), goat serum (2%), Triton-X-100 (0.5%) (Sigma, St Louis, MO, USA) at room temperature (RT). Then, the segments were incubated in a solution containing a 1:750 diluition of the rabbit serum containing the anti-myosin-V antibody in PBS, BSA (2%), Triton-X-100 (0.1%) and normal goat serum (2%) at RT for 24 h. After incubation, the tissues were rinsed twice in PBS Triton-X-100 (0.1%) and twice in the solution of PBS + Tween 0.05% (Sigma, St Louis, MO, USA). Segments were incubated in secondary antibodies (anti rabbit) conjugated with peroxidase 1:1,000 (Pierce, Rockford, USA) at RT, by shaking for 24 h. They were then rinsed 4 x 15 min, in PBS with 0.05% Tween-20. The tissues were developed with diaminobenzidine (DAB) (Sigma, St Louis, MO, USA) and mounted in glycerol gel. The negative control was performed with the lack of primary antibody.
Enteric neurons were counted using a BX 40 Olympus microscope with a 40x objective. Quantitative analysis was performed at the intermediate region (60° - 120°; 240° - 300°, with 0° as the mesenteric insertion) (Zanoni et al. 2005). Sixty microscope fields were randomly counted for each preparation. The area of each microscopic field was 0.229 mm2. The results were shown in cells.cm2.
For morphometric analysis of the myenteric neurons, images were taken with a high-resolution camera and sent to a microcomputer. The cell profile (µm2) of 100 cell bodies for each animal was measured through the image-analyses software Image-Pro-Plus 4, in a total of 500 neurons for each studied group. Neurons were classified by size into 100 µm2 bins and the percentage of each group was calculated for each bin.
Histological Procedure
Metaphasic index
Two hours prior the sacrifice, the animals were injected with 1 mg.Kg−1vincristine sulfate (Oncovin®, Eli Lilly, Brazil), a blocking agent of the mitotic spindle. The injections were always given at the same time of day to avoid circadian variations. Soon afterwards, the ileum was collected and carefully washed to remove the feces. The segments were opened along the mesenteric border, fixed with pins into a paper card with the mucosa surface upward. They were then immersed in buffered formalin for 6 hours.
After fixation, the ileum was dehydrated and embedded in 2-hydroxyethyl-metacrilate (Leica Historesine - Embedding Kit, Germany). Two micrometer semi-serial sections were made in a Leica RM 2145 microtome, with glass razor. The sectioned resins were stained by hematoxylin-eosin (HE).
The metaphasic index was calculated by counting the interphasic and metaphasic epithelial nuclei in the ileum crypts. Approximately 2,500 cells per animal were counted on BX 40 Olympus microscope under a 40 X lens. The metaphasic index was expressed as the percentage of nuclei in metaphase divided by the overall number of counted nuclei.
Goblet cells in the villus
Resins sectioned were stained using the pricro-indigo-carmin/periodic acid Schiff (PAS) histochemical technique to stain goblet cells. The number of stained goblet cells in one side of the villus and the picro-indigo-carmim/periodic acid-Schiff (PAS) method in one side of the villus and the overall number of cells on the same side of the villus were counted in all rats of each group. Approximately 2,500 cells per animal were counted - including positive or negative PAS - in longitudinal sections of intact villus (Hernandes et al. 2003) using BX 40 Olympus microscope under a 40 X lens. The number of goblet cells was expressed as the percentage of PAS-stained goblet cells divided by the overall number of counted cells.
Morphometry of villus and crypts
The height of the villus and the depth of the crypts were measured in well-guided longitudinal sections. The crypts depth measured as the distance between the junction crypt-villi and the crypt base. The length of the villus is measured as the distance between the crypt-villus junction and the villus apex. The morphometric assessment was carried out on 30 villus and 30 crypts per animal (150 measurements per group) using a 10x objective and an ocular with Zeiss micrometer grade.
Statistical analysis
The data were analyzed by the minimum squares method, through the Variance Analysis (ANOVA), followed by Tukey test, which was used as a post-test to compare the means. Since the areas of the cell bodies did not present a similar distribution, we employed the Variance Analysis and t-test to compare the means. The analyses were carried out with the software Prisma 3.0. The results are shown as means ± standard error (M ± SE).
RESULTS
Procedures Animals
We verified in this study that the diabetic rats (groups UD, DG4 and DG45) did not gain weight in the same proportion as the animals from the normoglycaemic groups (UN and NG) (P < 0.05) (Table I). The L-glutamine supplementation did not alter the final body weight of rats from groups DG4 and DG45 when compared to the animals from group UD (P > 0.05) (Table I). The diabetic condition was kept throughout the studied period, since glycaemia levels were high in all of the investigated diabetic groups. The diabetic syndrome was also verified by the polyphagia, polyuria, polydipsia and the L-glutamine supplementation did not alter these parameters (Table I).
TABLE I Glycaemia (GI), initial and final body weight (IBW and FBW), daily water consumption (DWC), daily food intake (DFI) and daily urine excretion (DUE) for animals belonging to the following groups: untreated normoglycaemic (UN), glutamine-treated normoglycaemic (NG), untreated diabetic (UD), glutamine-treated diabetic (DG4), glutamine-treated diabetic (DG45). All results are shown as means ± SE. n = 5 rats per group.
| Parameters | UN | NG | UD | DG4 | DG45 |
|---|---|---|---|---|---|
| GI mg.dl−1 | 158.1 ± 9.3a | 143.2 ± 7.1a | 649.6 ± 36.5b | 524.7 ± 44.8c | 500.5 ± 28.4c |
| IBW.g−1 | 330.6 ± 8.5a | 300.3 ± 9.3a | 314.8 ± 9.2a | 328.0 ± 8.2a | 312.4 ± 9.0a |
| FBW.g−1 | 480.3 ± 10.7a | 406.4 ± 13.4b | 309. 3 ± 17.7c | 292.1 ± 10.9c | 286.7 ± 18.5c |
| DWC.ml−1 | 54.35 ± 2.6a | 49.2 ± 1.35a | 185.7 ± 11.7b | 213.3 ± 7.0b | 160.6 ± 5.0b |
| DFI.g−1 | 32.1 ± 0.75a | 28.77 ± 1.1a | 50.8 ± 2.1b | 54.82 ± 1.2b | 48.3 ± 2.5b |
| DUE.ml−1 | 12.82 ± 1.7a | 10.7 ± 1.6a | 101.7 ± 5.5b | 127 ± 7.0c | 88.7 ± 3.8b |
Means followed by different letter on the same line are different by the test of Tukey (P < 0.05).
Myenteric Neurons
The myosin-V technique allowed us to observe the three components of the myenteric plexus (Fig. 1). The primary plexus was well evidenced, with the presence of ganglia and interganglionic nerve fibers. Isolated neurons were observed in the path of the nerve fibers of the primary plexus. The secondary and tertiary plexuses were also quite evident. The nerve fibers of the secondary plexus are parallel to the muscular cells of the circular layer of the muscular tunica. The tertiary plexus was formed by fine nerve fibers, situated between the spaces left by the primary plexus (Fig. 1). It was observed a different intensity in the neurons staining in the myenteric ganglions (Fig. 2).
Figure 1 Micrographs showing the components of the myenteric plexus of the ileum of rats stained by the myosin-V technique. Figure A e B: 1 – primary plexus; 2 – secondary plexus; 3 – tertiary plexus; 4 – isolated neurons. Calibration bar: (A) 50µm and (B)30µm.
Figure 2 Micrographs of the myenteric plexus of the ileum of rats showing myenteric ganglia stained by myosin-V belonging to animals from the groups: untreated normoglycaemic (A), L-glutamine-treated normoglycaemic (B), untreated diabetic (C), L-glutamine-treated diabetic (D), L-glutamine-treated diabetic (E). Calibration bar: 20µm
There was a 36.72% and 36.33% reduction in the neuronal density in the ileum of animals of group UD when compared to the untreated normoglycaemic (UN) and the normoglycaemic treated with L-glutamine (NG) respectively (P < 0.05). The neuronal density of animals of groups DG4 and DG45 was similar to that observed in the untreated diabetics (UD) (P > 0.05) (Fig. 3).
Figure 3 Density (Neurons/cm2) of myenteric neurons stained by myosin-V in the ileum of rats. Groups: untreated normoglycaemic (UN), glutamine-treated normoglycaemic (NG), untreated diabetic (UD), glutamine-treated diabetic (DG4), glutamine-treated diabetic (DG45). All results were shown as means ± standard error. n = 5 rats per group. *P < 0.05 when compared to group UN and NG.
The cell profile area of the myosin-V stained-neurons of animals of group UD was 4.6% larger when compared to the animals of group UN (P > 0.05) (Table II). The L-glutamine supplementation (group DG4 and DG45) did not change these results, with means similar to those of animals to group UD (P > 0.05). Most neurons had cell profiles that varied from 101 to 400 µm2. The proportion of neurons in this range for groups UN, NG, UD, DG4 and DG45 was of 82.2%, 89.6%, 84.4%, 92.2% and 88.4% respectively (Fig. 4).
Figure 4 Size distribution of myosin-V stained myenteric neurons. They were classified in classes of 100 µm2 for the animals in the groups: untreated normoglycaemic (UN), glutamine-treated normoglycaemic (NG), untreated diabetic (UD), glutamine-treated diabetic (DG4), glutamine-treated diabetic (DG45). n = 5 rats per group.
TABLE II Means and standard errors of the cell body areas of myosin-V stained neurons in groups: untreated normoglycaemic (UN), glutamine-treated normoglycaemic (NG), untreated diabetic (UD), glutamine-treated diabetic (DG4), glutamine-treated diabetic (DG45). n = 5 rats per group.
| Group | myosin-V |
|---|---|
| UN | 273.5 ± 17.17 |
| NG | 255.4 ± 5.268 |
| UD | 286.6 ± 11.59 |
| DG4 | 285.5 ± 21.16 |
| DG45 | 274 ± 12.91 |
Means did not have significant differences by the t- test (P > 0.05).
Metaphasic Index and Estimation of Goblet Cells in the Villus
The data related to the metaphasic index (Table III). The methafasic index of group UD was 23.2% higher when compared to group UN (P > 0.05). The treatment with L-glutamine (DG4 group) promotes a increase of 6.92% in metaphasic index in relation to the UD group (P > 0.05). The number of goblet cells of animals of groups UD, DG4 and DG45 was similar to those of animals of group UN and NG (P > 0.05) (Table III).
TABLE III Frequency of Goblet cells and metaphasic indexes of crypts of the ileum of rats belonging to groups in non-treated normoglycaemic rats (UN), L-glutamine-treated normoglycaemic (NG), non-treated diabetic (UD), L-glutamine-treated diabetic (DG4) and (DG45). All results were shown as means ± standard error. n = 5 rats per group.
| Grupo | Goblet Cells (%) | Index Metaphasic (%) |
|---|---|---|
| UN | 15.63 ± 0.441 | 6.792 ± 0.4207 |
| NG | 14.53 ± 1.273 | 8.326 ± 0.7619 |
| UD | 15.54 ± 0.955 | 8.856 ± 0.8805 |
| DG4 | 15.79 ± 0.798 | 8.843 ± 0.5702 |
| DG45 | 14.87 ± 0.733 | 7.586 ± 0.8120 |
There were no significant differences when the groups were compared by the test of Tukey (P > 0.05).
Morphometry of Villus and Crypts
Villus height in rats from groups DG4 and DG45 were 45.5% (P < 0.05) and 32.4% (P > 0.05) higher than those in group UD, respectively. The crypts of animals of group UD had a depth similar to those evidenced in the animals of group UN (P > 0.05). The crypt depth in DG4 and DG45 were 27.63% and 29.17% larger than in UD (P > 0.05), respectively. The means of the villi height (µm) and crypt depth (µm) (Fig. 5).
Figure 5 Villi height (µm) and crypts depth (µm) in the ileum mucosa of untreated normoglycaemic rats (UN), L-glutamine-treated normoglycaemic (NG), untreated diabetic (UD), L-glutamine-treated diabetic (DG4) and (DG45). All results were shown as means ± standard error. n = 5 rats per group.* P < 0.05 when compared to group UD.
DISCUSSION
Our experimental model of diabetes was effective because there was an increase on the daily water consumption, food intake and glycaemia. The animals of groups UD, DG4 and DG45 had a smaller body weight when compared to the normoglycaemic animals (groups UN and NG).
Myenteric neurons: The myosin-V immunohistochemical technique was used to stain the myenteric neurons in the muscular layer whole mounts (Drengk et al. 2000). Several authors have used this technique to stain myenteric neurons in different areas of the gastrintestinal tract (Buttow et al. 2003, 2004, Zanoni et al. 2003, 2005, Schoffen et al. 2005). Myosin-V is a versatile motor protein and it is involved in the fast transport of vesicles from the dendrites to the axon (Langford 2002). This technique is used as marker of the overall neural population because the myosin-V is present in cell bodies and nerve fibers (Drengk et al. 2000). With this technique, we are able to observe the organization of the myenteric plexus. We verified the presence of the three components that compose this plexus (primary, secondary and tertiary) similar to previous studies Furness and Costa (1980). The variable intestinity of imunoreactivity in the myenteric neurons inside the ganglia was observed in all studied groups. According to Drengk et al. (2000) heterogeneity of intensity may indicate different levels of neuronal activity.
We observed a 36.72% decrease on density of myenteric neurons stained by the myosin-V in group UD when compared to the normoglycaemic (UN). This result was similar to the one found byZanoni et al. (2003) and Alves et al. (2006) who verified a reduction in the neuron density in the ileum of diabetic rats. There are several factors that contribute to the reduction on the number of myenteric neurons. Some of them are: a) the increase of the aldose reductase activity, associated to an increase in the sorbitol and fructose levels (Ferraz et al. 1997); b) an increase in oxidative stress (Baynes 1991, Vincent et al. 2004) that causes an increment in the production of free radicals; c) a decrease in the levels of endogenous antioxidants. The glutathione levels are reduced during the hyperglycaemia leading to an increase in ROS (Parthiban et al. 1995, Greene et al. 1999, Vincent et al. 2004). Glutathione is an important antioxidant in most cells of mammals (Vincent et al. 2004). This substance serves as an essential cofactor for the glutathione peroxidase enzyme, which removes hydroperoxidase, and the formation of oxidized glutathione (GSSG). The reduced glutathione (GSH) is regenerated by the enzyme glutathione reductase using NADPH (Parthiban et al. 1995, Vincent et al. 2004). Therefore, the hyperactivity of the polyol pathway reduces the glutathione levels, causing an increase in the ROS (Nakamura 2002). This reduction is related to the increase of the aldose reductase activity that consumes NADPH, which is also necessary for the formation of the reduced glutathione (Tesfamariam 1994, Giugliano et al. 1996). All of these events involve an increase in oxidative stress and are related to the activation of a cascade of events that generate the apoptosis (Srinivasan et al. 2000, Barber 2003).
We hypothesized that L-glutamine supplementation in the DG4 group of animals would prevent the development of diabetic neuropathy. Furthermore, the objective of L-glutamine supplementation of the DG45 group of animals was to work as a treatment for diabetic. However, the L-glutamine supplementation was not efficient either in preventing or in treating this pathology at the dose used. L-glutamine is a very important energy substratum for cells, being also a precursor for nucleotides, glutamate and, especially, the GSH synthesis. This amino acid has its concentration reduced during the catabolic stress (Vincent et al. 2004). Studies carried out by Roth et al. (2002) showed that rats fed with L-glutamine had an increase in their cellular content of GSH. We observed that L-glutamine supplementation (DG4 and DG45) did not avoid the decrease on the number of myenteric neurons. This might be due to the fact that several mechanisms were producing ROS. Among them are: the polyol pathway, the autoxidative glucosilation, the reduction of antioxidants and the reduction of the efficiency of the enzymatic system (Vincent et al. 2004). Therefore, a combined treatment of substances already studied individually (as the ascorbic acid [Zanoni et al. 2003] or acetil-l-carnitine [Miranda-Neto et al. 2005]) with L-glutamine could be effective, because ROS would be neutralized by different mechanisms. We speculate that another factor to be questioned would be in relation to the concentration of used L-glutamine. In this experiment a concentration of 1% was used and could have been too small to produce the wanted biological effect. We worked with this concentration, because there is evidence in the literature that higher concentrations (4%) is harmful the intestinal mucous membrane (Shinozaki et al. 1997, Ameho et al. 1997). It is possible that an intermediate concentration could be beneficial to the neurons without damage to the intestinal mucous membrane.
There were no significant differences regarding the neuronal profile area when the five groups were compared. When comparing group UD with group UN, we observed that the immunoreactive neurons to myosin-V of animals belonging to UD were 4.6% larger than the animals from group UN. We have demonstrated previously Zanoni et al. (2003) that the cellular profile of myosin-V myenteric neurons of the ileum of diabetic rats was unaltered by treatment with ascorbic acid. On the other hand, we have also demonstrated that VIP-ergic and nitrergic neurons Zanoni et al. (2002, 2003 ) in the ileum had an increase in their area in diabetic rats and further, that ascorbic acid supplementation prevented this increase. We can infer that diabetes mellitus affects in a different way the subpopulations of myenteric neurons, since we have noticed no changes in the neuronal area when analyzing the neurons overall population and the suplementation with L-glutamine did not alter these results. When we analyze the distribution of the neuronal population in random classes at intervals of 100 µm2, we verified that despite the size variability observed in the area of the neuronal profile (47.301 to 855.102µm2), most neurons in both groups had a profile cell area ranging from 101 to 400 µm2. This shows the uniformity in the neuronal distribution between the groups.
Mucosa of the ileum: Our results did not show significant differences in the cell proliferation, crypts depth and villus height of the ileum mucosa at the end of 120th experiment day in UD when compared to UN and NG. Several studies have already shown changes in the small intestine of non-supplemented diabetic rats such as hyperplasia, hypertrophy of the mucosa (Miller et al. 1977, Zhao et al. 2003), increase on the crypts depth and villus heights after 4 days of diabetes in the duodenum and 7 days of diabetes in jejunum and ileum (Zhao et al. 2003). These results differ due to their use of a model of acute diabetes mellitus while our experimental model is of chronic diabetesmellitus. It is likely that the intestinal mucosa underwent an adaptation to the chronic pathogenesis of the diabetes mellitus. Data observed by Zoubi et al. (1995) did not find morphometric changes in the crypts depth and villus height in the small intestine of rats after 84 days of the diabetesmellitus onset.
The intestinal mucous membrane of the animals of the group DG4 presented an increase in the cellular proliferation in the proportion of 6.92% and an increase in 45.5% in the height of the villus when compared to the group UD. The villus in groups DG45 was 32.4% higher than those in group UD. The crypt depth in groups DG4 and DG45 were larger when compared to group UD (27.63% and 29.17% respectively). These results can be related the functional activity of L-glutamine which is considered the main energy source for the enterocytes (Fleming et al. 1997) to promote proliferation and cellular migration of the intestinal mucosa cells (Ruemmele et al. 1999). L-glutamine links to receptors at the luminal or basolateral surface of enterocytes and causes its own absorption (Palanch 2000). It is also possible that the villus suffered a delay in its cell death process, the L-glutamine may have prevented the villus apoptosis from happening because glutamine is a precursor of glutathione, which is reduced in intestinal mucosa due to the diabetesmellitus (Bhor et al. 2004). Previous studies have demonstrated that rats supplemented with L-glutamine (3%), for a period of 8 days, had an increased on the height of villus and number of mitotic cells per crypt after treatment with chemotherapeutics (Klimberg et al. 1990).
The number of goblet cells counts was similar among groups UD, UN, NG. A morphological study of the enteric epithelial mucosa of streptozotocin-induced diabetic rats, with 14 days of age has demonstrated similar number of goblet cells in the jejunum, ileum and duodenum Etharh and Carr (1997) or just ileum Mantle et al. (1989)when comparing the diabetic and control groups. In the present study, L-glutamine supplementation (groups DG4 and DG45) did not alter the number of goblet cells counts in the villus.
Summing up, the present work showed that the L-glutamine supplementation (1%) was not effective in altering the diabetes-induced loss of myenteric neurons, but promoted an increase of the size of the villus and depth of the crypts in the animals of the group DG4 and DG45. These results allow us to suggest that it is necessary new researches to prove the effectiveness of the suplementation with L-glutamine on the innervation enteric of the ileum of diabetic rats.
