Introduction
The influence of low birth weight due to intrauterine growth restriction (IUGR) on the susceptibility of developing metabolic disorders later in life has been documented in humans [1‐6]. The thrifty phenotype hypothesis proposes that malnutrition in early life can result in long-lasting alterations in structure and function of fetal tissues that are associated with the development of type 2 diabetes and metabolic syndrome at adulthood [7, 8]. Studies in rodent IUGR models have associated maternal caloric or protein restriction with hyperphagia and obesity in the adult offspring [9, 10].
The hypothalamus plays a crucial role in the maintenance of energy homeostasis and IUGR-induced hypothalamic disorders have been linked to obesity. A low protein diet throughout pregnancy and lactation induced morphological alterations in hypothalamic nuclei and high levels of hypothalamic neuropeptide Y (NPY) at weaning [11, 12]. Decreased expression of proopiomelanocortin mRNA levels in the hypothalamus of neonate rats whose dams were subjected to 50% caloric restriction has also been described [13].
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The effects of metabolic programming due to intrauterine malnutrition have been shown to be gender specific [14‐16]. We have previously shown that the IUGR-evoked alterations in the adult adipose tissue proteome were concordant with established obesity in female rats, while the males showed a metabolic status favoring later obesity development [17]. Our laboratory has also reported a more pronounced impairment of hypothalamic insulin action in female than in male rats submitted to IUGR [18].
We have recently shown deleterious consequences of IUGR in the hypothalamus of adult male rats. Impairment of glucose metabolism, respiratory chain and glutathione metabolism were observed, indicating alterations in mechanisms relevant to energy metabolism and redox homeostasis in this brain region at adulthood [19].
The current investigation, therefore, aimed at evaluating the long-term effects of IUGR, induced by calorie restriction, on the hypothalamus of female rats. Using a combined proteomics–metabolomics approach, we were able to identify potential pathways affected by undernutrition during pregnancy. The present results indicate that IUGR modified mechanisms related to GABAergic synapse, glutamate metabolism and TCA cycle in the hypothalamus of adult female rats.
Materials and methods
Animals
This study was approved by the Research Ethics Committee of the Universidade Federal de São Paulo—UNIFESP. Experimental procedures were conducted as described previously [19]. Briefly, pregnant 3-month-old female Wistar rats (Rattus norvegicus) were randomly assigned to be a control (fed ad libitum) or a restricted dam (fed 50% of control intake) throughout pregnancy. They were fed balanced chow (Nuvilab CR-1, Nuvital Nutrientes SA, Colombo, PR, Brazil) and kept under controlled light (12 h light:12 h dark cycle, lights on at 6 am) and temperature (22 ± 1 °C) conditions and had free access to water throughout the experimental period.
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After parturition, the offspring were weighed and litter size was adjusted to eight (four males and four females) per dam. Dams from both groups received food ad libitum during lactation. From weaning up to 4 months of age, female offspring was fed ad libitum. Food intake and body weight were evaluated once a week in the course of this period.
Sample collection
At 4 months of age, the rats were euthanized after 8 h of fasting; the hypothalamus was rapidly dissected and immediately frozen in liquid nitrogen. White fat depots (retroperitoneal, mesenteric and gonadal) were dissected and weighed. Trunk blood was collected and centrifuged at 1125×g for 20 min at 4 °C. Serum aliquots were stored at − 80 °C until further analysis.
Serum and tissue measurements
Glucose and triglycerides levels were determined using commercially available kits (Labtest Diagnóstica, Lagoa Santa, MG, Brazil). Serum leptin, insulin and adiponectin levels as well as hypothalamic levels of TNF-α, IL-6 and IL-10 were measured by Elisa (Millipore, Bedford, MA, USA). Briefly, the hypothalami (n = 6–8) were homogenized in 1 mL of chilled extraction buffer containing 100 mM Trizma Base pH 7.5, 10 mM EDTA, 100 mM NaF, 10 mM Na4P2O7, 10 mM Na3VO4, 2 mM PMSF, and 0.1 mg/ml aprotinin. After centrifugation at 20,800×g for 40 min at 4 °C, the supernatants were recovered and aliquots of 100 µL were used for protein assessment according to the manufacturer´s recommendations.
Proteomic analysis
Sample preparation
Extraction of hypothalamic proteins was performed as described previously [19]. Briefly, the whole frozen hypothalamus was homogenized in lysis buffer 8 M urea, 75 mM NaCl, 1 M Tris and complete Mini Protease Inhibitor Cocktail Tablets (Roche Diagnostics, Indianapolis, IN, USA) and protein concentration was determined (2-D Quant Kit, GE Healthcare, Waukesha, WI, USA). One milligram of sample protein was subjected to dialysis (Amicon Ultra-4 Centrifugal 3000 NMWL filter, Merck Millipore) against 50 mM ammonium bicarbonate. Then, 200 µg of concentrated protein were heated for 15 min at 80 °C in the presence of 25 µL of 0.2% RapiGest SF (Waters, Milford, MA, USA), reduced with 100 mM DTT, alkylated with 300 mM iodoacetamide and digested with trypsin (Promega, Fitchburg, WI, USA). The samples were then acidified with 5% trifluoroacetic acid, centrifuged and the supernatants transferred to the vials for MS analysis (Waters).
Mass spectrometry and data analysis
Hypothalamic samples (n = 4) were analyzed in triplicates on a nanoAcquity UPLC system coupled to a Synapt G2 HDMS Q-TOF mass spectrometer (Waters). Samples (5 µL) were loaded onto a trap column (nanoAquity C18 trap column Symmetry 180 µm × 20 mm, Waters) and transferred by an elution gradient (phase B gradient from 7 to 35% for 92 min at a 275 nL/min) through the analytical column (nanoAcquity C18 BEH 75 µm × 150 mm, 1.7 mm, Waters). The mobile phase A was 0.1% formic acid in water and the mobile phase B was 0.1% formic acid in acetonitrile. Data were acquired in data-independent mode (HDMSE), switching from low (4 eV) to high (ramped from 19 to 45 eV) collision energy. For external calibration, Glu-fibrinopeptide B solution (500 fmol/mL in 50% acetonitrile, 0.1 formic acid; Waters) was infused at 500 nL/min every 30 s using a nanoLockSpray apparatus.
Data were processed using the ProteinLynx Global Server software version 3.0.1 (Waters) with database search against Rattus norvegicus sequences in the UniProtKB/Swiss-Prot database (http://www.uniprot.org, including 9485 entries). The search parameters included automatic precursor and fragment mass tolerance, two missed cleavage sites allowed for trypsin digestion, cysteine carbamidomethylation as fixed modification and methionine oxidation, N-terminal acetylation, glutamine and asparagine deamidation as variable modifications. Additionally, the protein identification criteria included a minimum of one fragment ion per peptide, five fragment ions per protein and two peptides per protein. The false discovery identification rate was set at 4%. Label-free quantitative assessments based on peptide intensities were performed by integrating the intensities of the three most intense peptides of each identified protein [20]. Results were exported into Excel files and normalization was performed using the sum of protein intensities. For relative quantitation, only proteins identified in at least two technical replicates of at least three biological replicates were considered. Additionally, proteins not detected in any of the 12 replicates of one group (indicating that the intensities were below the detection limit), but identified in at least 4 replicates in the other group were listed and included in the pathway analysis.
Metabolomic analysis
Sample preparation
All procedures were carried out based on a previously described LC–MS/MS platform [21]. After whole hypothalamus homogenization (n = 8) in 500 µL of 80% precooled methanol, samples were incubated for 4 h at − 0 °C, centrifuged at 14,000×g for 10 min at 4 °C and the supernatant was collected. The remained pellet was mixed with 400 µL of 80% (v/v) methanol, followed by 30 min incubation at − 80 °C and a second centrifugation at the same conditions as described above. The combined supernatants were dried in a SpeedVac concentrator centrifuge (Thermo Fisher, Waltham, MA, USA). Extraction of serum metabolites was performed by mixing 200 µL of samples (n = 8) with 800 µL of precooled methanol. After incubation for 6 h at − 80 °C, samples were centrifuged at 14,000×g for 10 min at 4 °C and the supernatants dried in a SpeedVac.
Mass spectrometry and data analysis
Dried samples were reconstituted in 50% (v/v) acetonitrile. Methionine-d3 was used as an internal standard. The chromatographic separation was performed in an Agilent 1100 series HPLC system (Agilent Technologies, Santa Clara, CA, USA). Metabolites were separated using a 3.0 × 150 mm 3 µm Luna HILIC column (Phenomenex, Torrance, CA, USA). The mobile phase A was 5% acetonitrile, 20 mM ammonium hydroxide, 20 mM ammonium acetate (pH 9.0) and the mobile phase B was 100% acetonitrile. The gradient was 85–30% of phase B during 3 min and to 2% during 9 min. This condition was maintained for 3 min and increased back to 85% for 1 min. The column was reconditioned for 7 min before the next injection. The HPLC system was coupled to an ABSciex 5500 hybrid triple quadrupole mass spectrometer (Sciex, Framingham, MA, USA) operating with an electrospray ionization source (ESI) in positive/negative switch mode. The Q1 > Q3 transitions for positive/negative ion switching for the targeted metabolites were analogue to the analytical platform previously described [21, 22].
Raw data were extracted using the MarkerView v1.2.1 software (Sciex) to the following parameters: gaussian smooth width of 2 points, peak splitting factor of 5 points, one peak limited per chromatogram, a minimum intensity of 1000 cps, a minimum signal/noise ratio of 5 and a minimum peak width of 5 points. Retention time correction was performed based on methionine-d3. Only metabolites showing a single peak in the chromatogram were included in the analysis and the result tables were exported into Excel files. Normalization of hypothalamic metabolites was performed using the sum of intensities of all quantified metabolites while normalization of serum metabolites used methionine-d3 intensity.
Statistical analysis
Statistical analysis was performed in Statistica 12 Software (StatSoft, Tulsa, OK, USA). Body weight, white fat depots mass, food intake and serum and hypothalamic parameters are expressed as mean and standard error. Significance of the differences between the restricted and the control group was determined using Student’s t test. Statistical significance was set at p < 0.05.
Interaction network and pathway analysis
Interaction network of all proteins and metabolites affected by IUGR was generated using STITCH (http://stitch.embl.de/) [23], with confidence score fixed at 0.4 and no additional proteins allowed.
Pathway over-representation analysis was performed using the web server IMPaLA (http://impala.molgen.mpg.de/) [24]. Multiple testing correction was performed with the false discovery rate method (FDR, Benjamini–Hochberg) and significance was set to q ≤ 0.01.
Results
Body and fat depots mass, food intake and serum parameters
The body weight of the restricted group was significantly lower than that of the control group from birth (Table 1) until the eleventh week of age (data not shown). However, at 4 months of age, the body weight of the restricted group was no longer significantly decreased (Table 1).
Table 1
Body mass, food intake and fat depots mass of the control and restricted groups
Control | Restricted | |
|---|---|---|
Body weight at birth (g) | 5.93 ± 0.10 (12) | 4.99 ± 0.11*** (12) |
Body weight at weaning (g) | 84.77 ± 1.45 (12) | 71.75 ± 2.17*** (12) |
Body weight at 4 months (g) | 241.40 ± 3.92 (12) | 231.37 ± 3.37 (12) |
Food intake at 4 months (g/100 g) | 6.08 ± 0.15 (12) | 6.13 ± 0.17 (9) |
Retroperitoneal fat depot (g/100 g) | 0.84 ± 0.04 (12) | 0.94 ± 0.05 (12) |
Gonadal fat depot (g/100 g) | 2.46 ± 0.16 (12) | 3.01 ± 0.18** (12) |
Mesenteric fat depot (g/100 g) | 1.04 ± 0.04 (12) | 1.25 ± 0.06** (12) |
Fat depots sum (g/100 g) | 4.35 ± 0.22 (12) | 5.20 ± 0.22* (12) |
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Since weaning, there were no differences in food intake between the control and the restricted groups, except at the sixth and fourteenth weeks, when the restricted offspring ate 7% more and 5% less, respectively, than the controls (data not shown). As shown in Table 1, food intake was similar between the groups at 4 months of age.
The mass of gonadal and mesenteric white adipose tissues, as well as the sum of fat depots (retroperitoneal, gonadal and mesenteric), were significantly higher in the restricted than in the control group (Table 1).
A significant increase of glucose levels was detected in the restricted group while no significant differences were detected in serum insulin, triglycerides, leptin and adiponectin levels. Hypothalamic cytokine levels were similar between the groups (Table 2).
Table 2
Serum and hypothalamic parameters of the control and restricted groups at 4 months of age
Control | Restricted | |
|---|---|---|
Serum glucose (mg/dL) | 105.97 ± 3.86 (12) | 122.75 ± 4.90* (12) |
Serum insulin (ng/mL) | 0.44 ± 0.05 (7) | 0.50 ± 0.09 (7) |
Serum triglycerides (mg/dL) | 44.97 ± 3.10 (9) | 49.68 ± 5.46 (9) |
Serum leptin (ng/mL) | 3.84 ± 0.58 (10) | 3.90 ± 0.37 (10) |
Serum adiponectin (µg/mL) | 23.84 ± 3.37 (12) | 23.77 ± 5.20 (9) |
Hypothalamic TNF-α (pg/mL) | 45.96 ± 6.13 (8) | 49.69 ± 4.15 (8) |
Hypothalamic IL-6 (pg/mL) | 79.81 ± 4.79 (6) | 82.63 ± 6.34 (7) |
Hypothalamic IL-10 (pg/mL) | 134.63 ± 30.64 (8) | 114.40 ± 17.73 (8) |
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Proteomics
The female rat hypothalamus dataset comprised of 1475 proteins, each one identified by at least 2 peptides, with false discovery rate set to 4%. After application of the inclusion criteria for quantification (presence in at least 2 technical replicates and 3 biological replicates), 419 proteins were compared between the groups.
Table 3 shows the hypothalamic proteins significantly affected by IUGR. Ten proteins were down-regulated while 2 proteins were up-regulated in the hypothalamus of the restricted group. Additionally, 13 proteins were identified only in the control group, while 3 proteins were identified only in the restricted group. Glutamine synthetase, glutamate dehydrogenase 1 (mitochondrial) and glutamate decarboxylase 2, proteins which participate in glutamate–glutamine metabolism, were all down-regulated in the restricted group. Table S1 (supplementary material) details MS information on the proteins affected by IUGR.
Table 3
Hypothalamic proteins significantly affected by intrauterine growth restriction
UniProt ID | Gene name | Protein | Fold change (restricted/control) | p value |
|---|---|---|---|---|
Down-regulated by IUGR | ||||
Q05683 | Gad2 | Glutamate decarboxylase 2 | 0.49 | 0.0063 |
P30009 | Marcks | Myristoylated alanine-rich C-kinase substrate | 0.62 | 0.0422 |
Q9Z269 | Vapb | Vesicle-associated membrane protein-associated protein B | 0.62 | 0.0159 |
Q6Q0N1 | Cndp2 | Cytosolic non-specific dipeptidase | 0.68 | 0.0321 |
O35567 | Atic | Bifunctional purine biosynthesis protein PURH | 0.72 | 0.0072 |
P85969 | Napb | Beta-soluble NSF attachment protein | 0.74 | 0.0367 |
P09606 | Glul | Glutamine synthetase | 0.77 | 0.0368 |
P10860 | Glud1 | Glutamate dehydrogenase 1, mitochondrial | 0.77 | 0.0494 |
P70580 | Pgrmc1 | Membrane-associated progesterone receptor component 1 | 0.80 | 0.0244 |
Q62952 | Dpysl3 | Dihydropyrimidinase-related protein 3 | 0.92 | 0.0206 |
O08875 | Dclk1 | Serine/threonine-protein kinase DCLK1 | Not detected in the restricted groupa | |
P05696 | Prkca | Protein kinase C alpha type | ||
P16446 | Pitpna | Phosphatidylinositol transfer protein alpha isoform | ||
P18666 | Myl12b | Myosin regulatory light chain 12B | ||
P41562 | Idh1 | Isocitrate dehydrogenase [NADP] cytoplasmic | ||
P60522 | Gabarapl2 | Gamma-aminobutyric acid receptor-associated protein-like 2 | ||
P62198 | Psmc5 | 26S protease regulatory subunit 8 | ||
P62870 | Elob/Tceb2 | Elongin-B | ||
Q4V8E4 | Cfap36 | Cilia- and flagella-associated protein 36 | ||
Q62915 | Cask | Peripheral plasma membrane protein CASK | ||
Q66HR2 | Mapre1 | Microtubule-associated protein RP/EB family member 1 | ||
Q75Q39 | Tomm70 | Mitochondrial import receptor subunit TOM70 | ||
Q9R0I8 | Pip4k2a | Phosphatidylinositol 5-phosphate 4-kinase type-2 alpha | ||
Up-regulated by IUGR | ||||
P19234 | Ndufv2 | NADH dehydrogenase [ubiquinone] flavoprotein 2, mitochondrial | 1.24 | 0.0386 |
P27682 | Scg5 | Neuroendocrine protein 7B2 | 1.17 | 0.0275 |
O08775 | Kdr | Vascular endothelial growth factor receptor 2 | Not detected in the control groupb | |
P02688-2 | Mbp | Myelin basic protein (Isoform 2) | ||
P51146 | Rab4b | Ras-related protein Rab-4B | ||
Metabolomics
The analysis of the hypothalamic samples included 131 different metabolites that met the inclusion criterion (presence of a single chromatographic peak). Multiple reaction monitoring (MRM) transitions are shown in Table 4. The restricted group had decreased levels of 5 metabolites and increased levels of 2 metabolites in the hypothalamus when compared to the controls (Table 4). Among the hypothalamic metabolites altered by IUGR, 2 are involved in the TCA cycle (α-ketoglutarate and phosphoenolpyruvate) and 2 take part in purine metabolism (deoxyguanosine and guanosine).
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Table 4
Hypothalamic metabolites significantly affected by intrauterine growth restriction
KEGG entry | Metabolite | Single reaction monitoring Q1/Q3 | Fold change (restricted/control) | p value |
|---|---|---|---|---|
Down-regulated by IUGR | ||||
C03626 | ADMA (N,N-dimethylarginine) | 203.2/46.2 | 0.76 | 0.045 |
C00330 | Deoxyguanosine | 268.1/152.0 | 0.78 | 0.032 |
C00029 | UDP-d-glucose | 565.0/323.0 | 0.78 | 0.036 |
C00065 | Serine | 106.0/60.0 | 0.82 | 0.013 |
C00026 | α-Ketoglutarate | 145.0/101.0 | 0.87 | 0.049 |
Up-regulated by IUGR | ||||
C00387 | Guanosine | 284.1/135.0 | 1.31 | 0.020 |
C00074 | Phosphoenolpyruvate | 167.0/79.0 | 1.31 | 0.049 |
Interaction network and pathway analysis
The analysis showed significant enrichment of the interaction network of hypothalamic proteins and metabolites affected by IUGR (p = 0.00149). IUGR induced hypothalamic alterations were related to GABAergic synapse, alanine, aspartate and glutamate metabolism, TCA cycle, arginine biosynthesis, glyoxylate and dicarboxylate metabolism and HIF-1 signaling pathway (Table 5).
Table 5
Integrated pathway analysis of hypothalamic proteins and metabolites significantly affected by intrauterine growth restriction
Pathway | Protein | Metabolite | p value | q value |
|---|---|---|---|---|
GABAergic synapse | Glutamine synthetase (↓) | α-Ketoglutarate (↓) | 0.0000057 | 0.0012 |
Gamma-aminobutyric acid receptor-associated protein-like 2 (↓) | ||||
Protein kinase C alpha type (↓) | ||||
Glutamate decarboxylase 2 (↓) | ||||
Alanine, aspartate and glutamate metabolism | Glutamine synthetase (↓) | α-Ketoglutarate (↓) | 0.0000272 | 0.0037 |
Glutamate dehydrogenase 1, mitochondrial (↓) | ||||
Glutamate decarboxylase 2 (↓) | ||||
Citrate cycle (TCA cycle) | Isocitrate dehydrogenase [NADP] cytoplasmic (↓) | Phosphoenolpyruvate (↑) | 0.000286 | 0.0111 |
α-Ketoglutarate (↓) | ||||
Arginine biosynthesis | Glutamine synthetase (↓) | α-Ketoglutarate (↓) | 0.000326 | 0.0121 |
Glutamate dehydrogenase 1, mitochondrial (↓) | ||||
Glyoxylate and dicarboxylate metabolism | Glutamine synthetase (↓) | Serine (↓) | 0.00203 | 0.0369 |
α-Ketoglutarate (↓) | ||||
HIF-1 signaling pathway | Protein kinase C alpha type (↓) | α-Ketoglutarate (↓) | 0.0037 | 0.0432 |
Elongin-B (↓) |
Discussion
The existence of a relationship between low birth weight and the development of metabolic disturbances in adulthood has been established. In agreement with ours [17, 19, 25] and other reports [26, 27] in both genders, here we observed that 50% calorie restriction throughout pregnancy induced low birth weight of the female offspring. At adulthood, these restricted females had normal body weight but increased body fat, in accordance with earlier data [9, 28]. As adults, the restricted females were hyperglycemic with normal levels of insulin, indicating alteration of the glucose-insulin metabolism, a feature also previously reported as an IUGR effect [29‐31].
Since hypothalamic inflammation has been implicated as a relevant contributor to the development of obesity [32, 33], we investigated the inflammatory status of the hypothalamus and found no significant effects of IUGR on TNF-α, IL-6 and IL-10 tissue levels. Unlike these present cytokines results obtained in basal conditions, it has been previously demonstrated that IUGR increased the hypothalamic response of IL-1β, TNF-α and IL-6 mRNA to systemic lipopolysaccharide (LPS) challenge [34].
The hypothalamic proteome and metabolome profile indicated that IUGR affected GABAergic synapse, glutamate metabolism, and TCA cycle, all pathways that are highly interconnected.
The amination of α-ketoglutarate, a TCA intermediate, yields glutamate. Conversely, glutamate may generate α-ketoglutarate through the glutamate dehydrogenase reaction. In neurons and astrocytes, these reactions occur in a dynamic equilibrium, aimed at both assuring adequate levels of neurotransmitters and preventing impairment of the oxidative capacity of the cell and ATP depletion [35, 36].
IUGR down-regulated the levels of α-ketoglutarate, isocitrate dehydrogenase (the enzyme catalyzing the production of α-ketoglutarate in the TCA cycle), and glutamate dehydrogenase, indicating impaired α-ketoglutarate metabolism. In contrast, IUGR upregulated the levels of phosphoenolpyruvate (the precursor of pyruvate in glycolysis), possibly as a compensatory mechanism. Within neurons, anaplerotic carboxylation of pyruvate to yield oxaloacetate has been shown to compensate for the loss of α-ketoglutarate intrinsic to glutamatergic and GABAergic neurotransmission [37]. In the rodent cerebral cortex, a coupling between the rate of glucose oxidation and the flux of the GABA/glutamate–glutamine cycle has been demonstrated [38].
In the present study, the hypothalamic levels of the enzymes glutamine synthetase, and glutamate decarboxylase were down-regulated by IUGR. The excitatory neurotransmitter glutamate released by neurons undergoes uptake and conversion to glutamine by glutamine synthetase in astrocytes [35, 38]. Glutamine is released and transported back to neurons, where it acts as a precursor for the synthesis of glutamate by phosphate-activated glutaminase. Glutamate is decarboxylated to yield the inhibitory neurotransmitter γ-aminobutyric acid (GABA), a reaction catalyzed by glutamate decarboxylase in GABAergic neurons [39].
The current observation that IUGR affected GABAergic synapses and glutamate metabolism are in agreement with several lines of evidence in rodents. An association of IUGR, induced by either food deprivation or ligature of uterine vessels, and disturbances in the GABAergic system has been previously suggested by the finding of reduced glutamate decarboxylase activity in several brain regions [40, 41]. A proteomic approach has shown altered glutamate metabolism in the adult frontal cortex of a maternal low protein diet rat model [42]. We have previously shown that both hypothalamic and serum levels of glutamate were decreased in male rats submitted to IUGR [19]. Obesity and type 2 diabetes have also been associated with GABA/glutamate–glutamine cycle deregulation [43].
The roles of hypothalamic glutamate and GABA signaling in the control of energy balance have deserved attention. Studies in rodents have shown feeding stimulation by injection of glutamate agonists in the lateral hypothalamic area [44, 45] and impaired glucose homeostasis by inactivation of vesicular glutamate transporter in the ventromedial hypothalamus [46]. In vitro and in vivo studies have shown that hyperglycemia induced impairment of glutamate metabolism in neurons and astrocytes [47, 48].
The involvement of hypothalamic GABA signaling in the control of systemic glucose concentration has been previously demonstrated, as blockade of GABA receptors in the paraventricular nucleus increased plasma glucose concentrations [49]. Moreover, disruption of GABA release from a specific subset of non-AgRP non-POMC neurons of the arcuate nucleus of mice induced obesity through decreasing energy expenditure [50]. The present decrease in the hypothalamic expression of glutamate decarboxylase, reported as an indicator of GABA release [51], may be involved in the high plasma glucose and adiposity observed in female rats exposed to IUGR.
The relationship between disturbances of insulin and leptin signaling and disorders of the GABAergic synapse and glutamate metabolism in the hypothalamus of IUGR animals remains to be determined. Hypothalamic impairment of insulin and leptin actions due to IUGR has been previously shown by us and others [18, 52, 53]. Inactivation of insulin receptors in GABAergic neurons led to increased body weight and adiposity in female mice [54]. Moreover, leptin acts on GABAergic neurons to produce its anorexigenic effect [55] and also modulates glutamate uptake in hypothalamic astrocytes [56]. It is interesting to point out that here we observed decreased levels of UDP-glucose, which is a precursor of membrane glycosphingolipids. It has been demonstrated that glycosphingolipids-derived gangliosides take part in central leptin signaling and its neuronal deletion induces obesity in mice [57].
It has been reported that the changes induced by IUGR are gender-dependent [15‐18, 58, 59]. We have recently used the proteomics/metabolomics approach to examine the consequences of IUGR in the hypothalamus of adult male rats. The data indicated increased glucose levels and enhanced flux through the hexosamine pathway, along with effects on energy metabolism and redox homeostasis [19]. The findings presented herein strengthen the gender dimorphism in the response to IUGR. Interestingly, glutamate and GABA neuronal systems are sexually distinct in several hypothalamic nuclei, namely the medial preoptic area, the ventromedial nucleus and lateral area [60].
It has been shown in sheep that caloric restriction during pregnancy caused maternal hypoglycemia [61]. The ventromedial hypothalamic nucleus, whose GABAergic network is not fully developed before birth [62], has glucose-sensing neurons, which have been shown to be blunted by hypoglycemic episodes [63] and modulated by 17β-estradiol [64]. One might infer that glucose-sensing neurons in the ventromedial nucleus may be involved in the distinct responses to IUGR between genders.
In conclusion, the present results indicate that IUGR induced changes in hypothalamic GABA/glutamate–glutamine cycle of female rats, a derangement with potentially multiple consequences. The present data suggested obesity and hyperglycemia as results of the effect of IUGR on this pivotal neurotransmitters pathway.
Acknowledgements
This work was supported by the Brazilian agencies Conselho Nacional de Desenvolvimento Científico e Tecnológico—CNPq (Grant no. 478550/2009-0 to EBR) and Fundação de Amparo à Pesquisa do estado de São Paulo—FAPESP (Grants no. 2010/20268-0 to EBR and 2012/19321-9 to AKT).
Compliance with ethical standards
Conflict of interest
The authors declare that they have no conflict of interest.
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