- Research article
- Open Access
Age-dependent decrease in glutamine synthetase expression in the hippocampal astroglia of the triple transgenic Alzheimer's disease mouse model: mechanism for deficient glutamatergic transmission?
Molecular Neurodegeneration volume 6, Article number: 55 (2011)
Astrocytes are fundamental for brain homeostasis and the progression and outcome of many neuropathologies including Alzheimer's disease (AD). In the triple transgenic mouse model of AD (3xTg-AD) generalised hippocampal astroglia atrophy precedes a restricted and specific β-amyloid (Aβ) plaque-related astrogliosis. Astrocytes are critical for CNS glutamatergic transmission being the principal elements of glutamate homeostasis through maintaining its synthesis, uptake and turnover via glutamate-glutamine shuttle. Glutamine synthetase (GS), which is specifically expressed in astrocytes, forms glutamine by an ATP-dependent amination of glutamate. Here, we report changes in GS astrocytic expression in two major cognitive areas of the hippocampus (the dentate gyrus, DG and the CA1) in 3xTg-AD animals aged between 9 and 18 months. We found a significant reduction in Nv (number of cell/mm3) of GS immunoreactive (GS-IR) astrocytes starting from 12 months (28.59%) of age in the DG, and sustained at 18 months (31.65%). CA1 decrease of GS-positive astrocytes Nv (33.26%) occurs at 18 months. This Nv reduction of GS-IR astrocytes is paralleled by a decrease in overall GS expression (determined by its optical density) that becomes significant at 18 months (21.61% and 19.68% in DG and CA1, respectively). GS-IR Nv changes are directly associated with the presence of Aβ deposits showing a decrease of 47.92% as opposed to 23.47% in areas free of Aβ. These changes in GS containing astrocytes and GS-immunoreactivity indicate AD-related impairments of glutamate homeostatic system, at the advanced and late stages of the disease, which may affect the efficacy of glutamatergic transmission in the diseased brain that may contribute to the cognitive deficiency.
The central nervous system relies on astrocytes for its correct functioning. Astroglia is critical for metabolic support to neurones by providing glucose and lactate [1, 2], regulates ion environment, i.e. K+ and water movements and provides reactive-oxygen-species scavengers like glutathione [3–5].
Astrocytes, as a component of the tripartite synapse, modulate neurotransmission and control the extracellular level of neurotransmitters [6–11]. Therefore, astrocytes are essential for glutamatergic transmission being key elements for "de novo" synthesis of glutamate and for the glutamate-glutamine cycle; which, in addition, are fundamental for the synaptic plasticity associated to cognitive processes [12, 13]. The bulk of glutamate release during neurotransmission is taken up by astroglia through Na+-dependent glutamate transporters [9, 14]. In astrocytes glutamate is converted to glutamine by glutamine synthetase (GS)  (which is considered astrocytic-specific enzyme although some recent studies have shown some degree of oligodendroglial and microglial GS expression under some pathological situations [15, 16]). Subsequently, astrocytic glutamine is transported back to neurones for its further conversion into glutamate [9, 17]. Thus, the glutamate-glutamine shuttle makes both astrocytes and GS essential for glutamatergic neurotransmission . At the same time astrocytic glutamate uptake prevents glutamate excitotoxicity ; disturbance of astroglial-based glutamate homeostasis may lead to neurotransmitter imbalance, neuronal malfunction and death, as well as impaired cognition [18, 19].
Astroglia is fundamental for the onset, progression and outcome of neuropathological processes by limiting the damage and promoting the revascularisation of the surrounding tissue through reactive astrogliosis [20–23] and by contributing to neuroinflammation by release of various pro-inflammatory factors, such as interleukins [24–26].
Alzheimer's disease (AD) is a highly malignant neurodegenerative process characterised by anomalous intraneuronal and extracellular accumulation of β-amyloid protein (Aβ)  and hyperphosphorilated cytoskeletal Tau protein in neurons . As a consequence of this anomalous protein formation and by a yet unknown mechanism, severe loss of specific ACh neurons and synapses appear at middle and advanced stages of the disease . As a result, the CNS reacts by both neuronal compensation and glial reactivity [30, 31]. Recently, in a GFAP based study, we have described that the associated reactive astrogliosis observed in the triple transgenic animal model (3xTg-AD) is preceded by a generalized atrophy of astrocytes that occurs at the middle stages of the disease (9-12 months of age). Formation of the senile plaques triggers secondary astrogliosis in astrocytes associated with Aβ depositions, and the later stages of the pathology are characterized by concomitant astroglial atrophy and astrogliosis that in any case is not associated with astrocytic density alterations (12-18 months of age) [32, 33]. Furthermore, and even if the two main pathological hallmarks have to be considered when studying AD, astrocytic involvement, as recently demonstrated by us [32, 33], is mainly related with Aβ pathology, since astrocytes modulate extracellular volume and components and Aβ directly affects the extracellular space, while tau pathology remains intraneuronal throughout AD .
Materials and methods
All animal procedures were carried out in accordance with the United Kingdom Animals (Scientific Procedures) Act of 1986 under the license from the Home Office. All efforts were made to reduce the number of animals by following the 3R's.
Experiments were performed on male 3xTg-AD mice, which harbours the mutant genes for amyloid precursor protein (APPSwe), for presenilin 1 PS1M146 V and for tauP301 L [34, 35] and their background-matching controls as described in detail previously [34–37].
Fixation and tissue processing
Animals of different age groups (9, 12 and 18 months; n = 4-8) were anaesthetized with intraperitoneal injection of sodium pentobarbital (50 mg/kg). Mice were perfused through the aortic arch with 3.75% acrolein (25 ml, TAAB, UK) in a solution of 2% paraformaldehyde (Sigma, UK) and 0.1 M phosphate buffer (PB) pH 7.4, followed by 2% paraformaldehyde (75 ml). Brains were then removed and cut into 4 - 5 mm coronal slabs of tissue consisting of the entire rostrocaudal extent of the hippocampus, as described previously . The brain sections were post-fixed in 2% paraformaldehyde for 24 hours and kept in 0.1 M PB, pH 7.4. Coronal sections of the brain were cut into 40 - 50 μm thickness using a vibrating microtome (VT1000 S, Leica, Milton Keynes, UK). Free floating brain sections in 0.1 M PB, pH 7.4 were collected and stored in cryoprotectant solution containing 25% sucrose and 3.5% glycerol in 0.05 M PB at pH 7.4. Coronal vibratome sections at levels -1.58 mm/-2.46 mm (hippocampus) posterior to Bregma, were selected for immunohistochemistry according to the mouse brain atlas of Paxinos and Franklin .
A mouse antiserum generated against GS (anti-GS; Millipore, UK; MAB302) was used for the determination of GS positive astrocytes. A rabbit anti-GFAP IgG fraction of antiserum (Sigma-Aldrich, UK; #G9269) was used for the determination of glial cytoskeleton and comparison to GS labelling distribution. A monoclonal antibody against amyloid beta conjugated with alexa 488 (Convance, USA; SIG-39347) was employed to label neuritic plaques. The immunolabelling pattern that we obtained with these antibodies is equivalent to that obtained previously [32, 39] and their specificity has also been previously demonstrated by western blot [36, 40–42]. To assess for non-specific background labelling or cross reactivity between antibodies derived from different host species, a series of control experiments were performed. Omission of primary and/or secondary antibodies from the incubation solutions resulted in a total absence of target labelling (data not shown).
To minimise methodological variability, sections through the dorsal hippocampus containing both hemispheres of all animals were processed at the same time using precisely the same experimental conditions. For this procedure, the vibratome sections were first incubated for 30 min in 30% methanol in 0.1 M PB and 3% hydrogenperoxide (Sigma, UK). Sections were rinsed with 0.1 M PB for 5 mins and placed in 1% sodium borohydride (Aldrich, UK) for 30 minutes. Subsequently the sections were washed with PB profusely before rinsing in 0.1 M TS for 10 minutes. Brain sections were then incubated with 0.5% albumin bovine serum (BSA, Sigma, Dorset, UK) in 0.1 M TS and 0.25% Triton X-100 (Sigma, Dorset, UK,) for 30 minutes. For the single labelling, sections were incubated for 48 hours at room temperature with primary antibody (mouse anti-GS, 1:500, cat# MAB302, Millipore, UK). The sections were rinsed in 0.1 M TS for 30 minutes and incubated in 1:200 dilution of biotinylated horse anti-mouse IgG (Vector laboratories, Peterborough, UK) for 1 hour at room temperature. Sections were rinsed in 0.1 M TS for 30 minutes, followed by incubation for 30 minutes in avidin-biotin peroxidase complex (Vetor Laboratories Ltd, Peterborough, UK). The peroxidase reaction product was visualized by incubation in a solution containing 0.022% of 3,3'diaminobenzidine (DAB, Aldrich, Gilligham, UK) and 0.003% H2O2 for 1.5 minutes as described previously [36, 37]. The reaction was stopped by rinsing the tissue in 0.1 M TS for 6 minutes followed by 0.1 M PB for 15 minutes. Brain sections were permanently mounted onto gelatinized slides. Sections were then dehydrated in ascending concentration of ethanol (50, 70, 80, 90, 95 and 100%) followed by xylene; and then permanently coverslipped.
For dual immunofluorescence labelling, the sections were incubated for 48 h at room temperature in primary antibody cocktail containing: (1) mouse anti-GS (1:500) and (2) rabbit anti-GFAP (1:30,000) simultaneously. Subsequently, GS and GFAP were detected in a sequential manner on the same sections by incubation with Alexa Fluor 594-conjugated goat anti-mouse and Alexa Fluor 488-conjugated goat anti-rabbit (Invitrogen, Paisley, UK), respectively.
For triple immunofluorescence labelling, the sections were incubated for 48 h at room temperature in primary antibody cocktail containing: (1) mouse anti-GS (1:500) and (2) rabbit anti-GFAP (1:30,000) simultaneously. Subsequently, GS and GFAP were detected in a sequential manner on the same sections by incubation with Alexa Fluor 594-conjugated goat anti-mouse and Alexa Fluor 633-conjugated goat anti-rabbit (Invitrogen, Paisley, UK), respectively. Then, the sections were washed in 0.1 M TS for 30 min and incubated in 0.5% BSA in 0.1 M TS and 0.25% Triton X-100 for 30 minutes. Subsequently, sections were incubation in mouse anti-amyloid beta Alexa 488-conjugated antibody (1:2000) for 20 hours at room temperature.
Finally, in both dual and triple immunoflorescence labelling, sections were rinsed with 0.1 M TS for 30 min and permanently mounted in an aqueous medium (Vectashield; Vector laboratories, Peterborough, UK).
GS positive cell count in hippocampus
We determined the numerical density (Nv; #/mm3) of GS positive astrocytes at 9, 12 and 18 months of age in both 3xTg-AD and non-Tg mice in the DG and CA1 subfields of the hippocampus. For this, 3 - 4 representative non-consecutive coronal sections throughout the dorsal hippocampus at levels -1.70/-2.18  were quantified accounting for an analyzed volume of approximately 6,000,000 μm3 in the DG and 15,000,000 μm3 in CA1. The specific analysed areas were the molecular layer (MoL) in the DG and all the strata of the CA1 apart from the pyramidal cell layer that is practically devoid of GS expression due to the dense packing of pyramidal somata and almost no presence of astrocytic cell bodies. GS positive astrocytes were intensely labelled against lighter background that made them easy to identify with equal chance of being counted. A single observer determined the number of GS positive astrocytes blindly; therefore, counting bias was kept to a minimum.
Optical Density (OD) Measurement
Using computer-assisted imaging analysis (Image J 1.32j, NIH, USA), we analyzed the expression and density of GS labelling at 9, 12 and 18 months of age in both 3xTg-AD and non-Tg mice by measuring their optical density (OD) as described previously . Briefly, to exclude any experimental errors and/or bias, all images were taken at constant light intensity. Optical filters were used to ensure the specificity of the signal recorded by the camera. The staining was observed throughout the thickness of the section (40 μm) using light microscopy (Nikon Eclipse 80i). No differences were observed in GS immunoreactivity throughout the thickness of the section between 3xTg-AD and non-Tg control animals; hence the changes in OD were used as measure of increased GS expression. The OD was calculated from a relative scale of intensity ranging from 0 to 255, with readout of 250 corresponding to the area with very low GS expression and 0 corresponding to the densest area of labelling. The calibration density was kept constant for measuring all section to avoid experimental variances. Sections background OD was determined from the corpus callosum (CC) that was considered as blank since GS labelling in the CC is virtually absent. GS density of the entire DG MoL and CA1 (with the exception of the pyramidal cell layer) were measured independently and a single measurement was obtained from every sub-region in each hemisphere. To analyze the change in GS density against constant control, the 255 was divided by control region (CC) and the obtained factor was multiplied by the region of interest in every given section. Inverse optical density was obtained by subtracting from the obtained background level (set at 255). Measurement of mean density were taken and averaged, after background subtraction, from each hippocampal layers in both the left and the right hemisphere of each slice. The results are shown as inverse GS density (IOD/pixel).
GS and GFAP positive cell count in relation to Aβ plaques in CA1
Triple labelling pictures of the CA1 at 18 months of age in both 3xTg-AD and non-Tg mice were taken using confocal scanning microscopy (Leica SP2, inverted), recording layers at every 0.5 μm. Both GS and GFAP positive cells were counted separately and taking in to account their localisation regarding Aβ plaques. We considered all cells with the somata within 50 μm from the plaque border of the plaque-associated, and cell with somata positioned more distantly as cells not associated with plaques.
Data were expressed as mean ± SEM. Unpaired t-tests were used to examine differences between 3xTg-AD and non-Tg animals at different time points and differences between away and around conditions in 3xTg-AD. Significance was accepted at p ≤ 0.05. The data were analyzed using GraphPad Prism (GraphPad Software).
GS immunoreactive (GS-IR) astrocytes were widely distributed throughout the subdivisions of the hippocampus in both non-Tg and 3xTg-AD mice. This distribution was similar to the GFAP immunoreactivity in both DG and CA1 (Figure 1C, E, G, 2A). GS-IR astrocytes show typical protoplasmic morphology characterized by small round cell bodies with few primary and several secondary processes extending radially in random fashion. GFAP-IR astrocytes were characterised by primary and secondary cytoskeleton processes extending radially from the cell body and frequently co-localising with GS-IR main processes. (Figure 1A, B, D, F, H). However, and differently to GFAP-positive astrocytes, GS-IR astrocytes showed a clear and profuse labelling not only in the cell body and primary processes but also throughout the fine and thin distal processes (Figure 1A, D, 3C-F).
GS immunoreactivity in non-Tg animals
In non-Tg animals, GS-IR showed a uniform pattern in the DG and in the CA1 being constant at all age groups. The GS-IR Nv at all ages was significantly lower in the DG compared to the CA1 (5,599 ± 603 cells/mm3 vs. 9,700 ± 1,041 cells/mm3, 42.27%, p = 0.009; 4,852 ± 306 cells/mm3 vs. 10,456 ± 1,788 cells/mm3, 53.59%, p = 0.021; 5,064 ± 511 cells/mm3 vs. 10,727 ± 1,083 cells/mm3, 52.78%, p = 0.001; at 9, 12 and 18 months respectively; Figure 3A, B). The overall GS-IR, as determined by the IOD, was slightly higher in the DG at 9 and 12 months of age when compared to CA1 (10.67% and 14.38%); but just being significantly higher in the advanced age (18 months, 16.34%, p = 0.046; Figure 4A, B).
Nv of GS-IR astrocytes decreases in 3xTg-AD mice
From 12 months of age the 3xTg-AD mice showed a significant reduction of the Nv of GS-IR cells in the DG (4,852 ± 306 cells/mm3 vs 3,465 ± 344 cells/mm3; 28.59%, p = 0.016; Figure 3A) compared to the non-Tg control animals, whereas no apparent difference was found in CA1. At 18 months of age the decrease in GS-IR cell Nv was significant in both the DG (5,064 ± 511 cells/mm3 vs 3,462 ± 321 cells/mm3; 31.65%, p = 0.036) and in the CA1 (10,727 ± 1083 cells/mm3 vs 7,159 ± 400.78 cells/mm3; 33.26%, p = 0.026; Figure 2, 3C-3F).
3xTg-AD mice exhibit a decrease in GS expression
In parallel to the decrease in the Nv of GS-IR cells, we observed a decrease in the expression of GS in the hippocampus with no apparent regional differences, as shown by the decrease of the inverse optical density (IOD; Figure 4). The 3xTg-AD mice, when compared to non-Tg controls, showed a significantly decreased GS expression in both DG (66 ± 3 vs 52 ± 4; 21.62%; p < 0.05) and CA1 (57 ± 2 vs 46 ± 2; 19.69%; p = 0.010) at 18 months of age (Figure 4), but not at the earlier ages (Figure 4A, B).
Nv of GS-IR astrocytes decrease in 3xTg-AD mice is associated, although no exclusive, with Aβ plaques
GS-IR decrease was not homogenous throughout the CA1 parenchyma in 3xTg-AD. GS-IR Nv was compared with GFAP-IR Nv in either the vicinity or distant of Aβ plaques in 3xTg-AD at 18 months of age, to asses whether GS expression changes were related to Aβ plaques. No GFAP-IR Nv related changes were observed in any of the conditions (Figure 5). However, GS-IR astrocyte Nv was significantly diminished in CA1 areas free of Aβ (10,069 ± 572 cells/mm3 vs 7,704 ± 558 cells/mm3; 23.49%, p = 0.010) when compared to GFAP-IR Nv density in same areas, being this reduction more patent in the vicinities of neuritic plaques (10,314 ± 922 cells/mm3 vs 5,338 ± 685cells/mm3; 48.24%, p = 0.002). In addition, GS-IR Nv associated to neuritic plaques was significantly lower to GS-IR Nv away from Aβ deposits (by 24.24%, p = 0.022).
GS-IR and GFAP-IR Nv was almost identical in non-Tg controls, showing 99.22% of co-localisation (data not shown).
In the present study we analysed the functional status of astroglia in the triple transgenic AD animal model by determining the expression of the GS at different ages. Our results in this animal model demonstrate that the expression of astroglial GS in hippocampus is affected at the human equivalent advanced and late stages of AD, as indicated by a reduction in both the Nv of GS-IR astrocytes and GS expression (as determined by IOD) in the 3xTg-AD when compared to the control animals. These changes in Nv appear in both DG and CA1, albeit they initially occur in the DG at 12 months of age. Such reduction becomes more evident in the surroundings of Aβ plaques at 18 months of age. The GS expression is also decreased in the 3xTg-AD in both DG and CA1 but at a later age (18 months).
Astrocytes are known to be involved in most neurological diseases including AD [20, 22, 33]. AD is characterised by a profound cognitive impairment due to a severe loss of synapses and neurones; which is generally believed to be associated with reactive astrogliosis [28, 44]. Our recent studies in the 3xTg-AD animal model, however, have found a more complex astroglial reactions in the late stages; which might show a similar pattern during human AD progression. At the early stages of the pathology astrocytes undergo generalised atrophy and down-regulation of GFAP expression, which may indicate early compromise of astrocytic homeostatic functions [23, 32, 33]. Several studies have previously described that GFAP abnormalities are associated with impaired glutamate homeostasis [45–48]. In a hypoxic animal model, astrocytes in the affected areas showed an abnormal GFAP cytoskeleton characterised with very short processes; which was associated with redistribution of GFAP and GLAST to the cell body, suggesting an impaired glutamate homeostasis . In addition, in GFAP knock-out mice, the lack of GFAP compromised the trafficking of the GLT-1 to the cell membrane, affecting glutamate uptake . Furthermore, "in vitro" studies have shown an inverse correlation between astroglial expression of GFAP and GS . Recently has been demonstrated that, as opposed to what was thought, 3xTg-AD model shows some degree of neuronal loss as a consequence of the pathological burden , strengthening the relevance of this AD model and allowing the comprehension of many described synapse-related pathological events like the current one.
Studies in AD brains have shown a decrease of cortical astrocytic GS expression [50, 51] that is accompanied by a "de novo" neuronal expression of GS as a compensatory reaction [51, 52]. This direct effect on astrocytic GS expression is also present in other neurodegenerative diseases, such as Huntington's disease, which is associated with GLT-1 glutamate transporter down-regulation [53, 54]. Further studies show that GS is oxidized due to Aβ in AD brains causing reduction of enzymatic activity  and that GS reduced expression is related to neuritic plaques in AD brain cortex . On the contrary, human studies have shown increased levels of GS immunoreactivity in the prefrontal cortex in AD brains . Obviously, phylogenetic proximity, tissue preservation and medical history play crucial role in the interpretation of human vs rodent data. Our current work shows that astrocytes at the late stages (plaque formation and stabilisation, 12-18 months) of AD-like pathology, in agreement with the above-mentioned studies, are functionally compromised as shown by the reduction of GS expression and therefore their capability to master the glutamate-glutamine cycle.
Thus, we could hypothesise that astrocytes fail to support neurones and control synapses from the appearance of the disease pathological burden. Furthermore, and considering astrocytic physiological function, one could consider that these changes result in an impaired glutamate homeostasis that is manifested by deficient glutamate/glutamine turnover and restricted supply of glutamine to neurones, being this failure somehow more dramatic in the proximities of Aβ plaques. Furthermore, GS deficiency could also be a consequence of impaired astrogial glutamate uptake; inducing a potential neurotoxic process by abnormal glutamate metabolism. Hence GS deficiency may reflect an altered glutamatergic neurotransmission of AD, at the advanced and late stages of the disease, which can account for a global hippocampal neurotransmitter imbalance underlaying the mnesic and cognitive impairments observed in the disease.
Triple transgenic mouse of Alzheimer's disease
- ACh neurons:
Cornus ammonis 1
Central nervous system
Dentate gyrus; GcL Granule cell layer
Glial fibrillary acidic protein
Glutamate aspartate transporter
Glutamine synthetase immunoreactivity/-reactive
Inversed optical density
Stratum lacunosum moleculare
Numerical density (cell number/mm3)
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The present study was supported by Alzheimer's Research Trust Programme Grant (ART/PG2004A/1) to JJR and AV. Grant Agency of the Czech Republic (GACR 309/09/1696 and GACR 304/11/0184) to JJR and (GACR 305/08/1381; GACR 305/08/1384) to AV. The Spanish Government, Plan Nacional de I+D+I 2008-2011 and ISCIII- Subdirección General de Evaluación y Fomento de la investigación (PI10/02738) to JJR and AV and the Government of the Basque Country grant (AE-2010-1-28; AEGV10/16) to JJR. The authors would also like to thank BBSRC for the Ph.D. studentship to H.N. Noristani.
The authors declare that they have no competing interests.
MO carried out the immunohistochemical study and contributed to the writing of the manuscript. HNN contributed to the immunhistochemical study. AV participated in the conception of the study and writing. JJR participated in the conception and design of the study and writing of the manuscript as well as coordinated the study. All authors read and approved the final manuscript.