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. 2011 Dec 19;3(5):e00071. doi: 10.1042/AN20110025

Early astrocytic atrophy in the entorhinal cortex of a triple transgenic animal model of Alzheimer's disease

Chia-Yu Yeh *, Bhamini Vadhwana †, Alexei Verkhratsky *,‡,§,║,, José J Rodríguez ‡,§,║,¶,1
PMCID: PMC3243908  PMID: 22103264

Abstract

The EC (entorhinal cortex) is fundamental for cognitive and mnesic functions. Thus damage to this area appears as a key element in the progression of AD (Alzheimer's disease), resulting in memory deficits arising from neuronal and synaptic alterations as well as glial malfunction. In this paper, we have performed an in-depth analysis of astroglial morphology in the EC by measuring the surface and volume of the GFAP (glial fibrillary acidic protein) profiles in a triple transgenic mouse model of AD [3xTg-AD (triple transgenic mice of AD)]. We found significant reduction in both the surface and volume of GFAP-labelled profiles in 3xTg-AD animals from very early ages (1 month) when compared with non-Tg (non-transgenic) controls (48 and 54%, reduction respectively), which was sustained for up to 12 months (33 and 45% reduction respectively). The appearance of Aβ (amyloid β-peptide) depositions at 12 months of age did not trigger astroglial hypertrophy; nor did it result in the close association of astrocytes with senile plaques. Our results suggest that the AD progressive cognitive deterioration can be associated with an early reduction of astrocytic arborization and shrinkage of the astroglial domain, which may affect synaptic connectivity within the EC and between the EC and other brain regions. In addition, the EC seems to be particularly vulnerable to AD pathology because of the absence of evident astrogliosis in response to Aβ accumulation. Thus we can consider that targeting astroglial atrophy may represent a therapeutic strategy which might slow down the progression of AD.

Keywords: Alzheimer's disease, astrocyte, dementia, entorhinal cortex, glial fibrillary acidic protein (GFAP), memory

Abbreviations: AD, Alzheimer's disease; Aβ, amyloid β-peptide; EC, entorhinal cortex; GFAP, glial fibrillary acidic protein; GFAP-IR, glial fibrillary acidic protein-immunoreactive; HC, hippocampus; LEC, lateral entorhinal cortex; NFT, neurofibril tangle; non-Tg, non-transgenic; Nv, numerical density; PB, phosphate buffer; PHF, paired helical filament; RT, room temperature; SP, senile plaque; 3xTg-AD, triple transgenic mice of AD; TS, Tizma-based saline

INTRODUCTION

The EC (entorhinal cortex), a part of the temporal cortex, is involved in mnesic processes by establishing the cortico-hippocampal circuits. The EC is divided into superficial (I–III) and deep layers (IV–VI) that show differential anatomical and functional organization (Suzuki and Amaral, 1994; Witter and Amaral, 2004). The superficial layers are the main recipient of intracortical information and the major output source to the HC (hippocampus), whereas the deep layers are mainly responsible for the projections to cortical regions (Figure 1; Suzuki and Amaral, 1994; Witter and Amaral, 2004). The neurons from the EC layer II terminate in the middle and outer molecular layer of the DG (dentate gyrus) and send collaterals to the hippocampal CA2 and CA3 fields (Witter et al., 1989; Tamamaki and Nojyo, 1993; Suzuki and Amaral, 1994). Layer III neurons project mainly to the CA1 and subiculum, which in turn feedback to layer V of the EC (Naber et al., 2001). Functionally, activation of the EC and persistent neuronal activity in the EC are involved in the process of working memory (Ranganath et al., 2003; Fransen, 2005; McGaughy et al., 2005). The EC is also essential for memory consolidation (Remondes and Schuman, 2004; Craig and Commins, 2005) and spatial navigation and memory (Fyhn et al., 2004; Moser et al., 2008).

Figure 1. Schematic illustration of entorhinal inputs to the HC.

Figure 1

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In brief, the superficial layers (I–III) project to the hippocampal formation and subiculum, while the deep layers (V/VI) receive reciprocal inputs from these areas. Meanwhile, deep layers also innervate to parahippocampal areas and the HC.

Entorhinal dysfunction is involved in several brain diseases that compromise cognitive and memory functions, including AD (Alzheimer's disease) (Braak and Braak, 1991; Kril et al., 2002; Schwarcz and Witter, 2002; Cunningham et al., 2006). The AD is an irreversible neurodegenerative disease accompanied by cognitive/memory impairments, which is the most common cause of progressive dementia in elderly people (Braak and Braak, 1991; Braak et al., 1999; Harciarek and Jodzio, 2005). AD is characterized by the appearance of SPs (senile plaques) representing extracellular Aβ (amyloid β-peptide) depositions (Nagele et al., 2004) and NFTs (neurofibril tangles) consisting of abnormally hyperphosphorylated tau protein, the latter being a major microtubule-associated protein (Schneider and Mandelkow, 2008). The EC is affected very early by AD pathology; it is arguably the first brain region experiencing Aβ accumulation (Braak and Braak, 1991, 1997; Thal et al., 2000). Similarly, the NFTs appear in the transentorhinal region and in the EC at the early stages of AD (Braak stages I/II) and are widespread in the EC at middle Braak stages (limbic stages III/IV) (Solodkin et al., 1996; Braak and Braak, 1997). Concomitant with the presence of Aβ and NFTs in the EC, this cortical region undergoes severe volume decrease that also affects its major projection target, the HC (Du et al., 2001; Halliday et al., 2003; Whitwell et al., 2008). Profound neuronal loss, mainly in layer II, also occurs in AD concomitantly with mild cognitive impairment (Gomez-Isla et al., 1996; de Toledo-Morrell et al., 2000; Du et al., 2001; Rodrigue and Raz, 2004).

The AD-related neuronal loss and atrophy of the EC are well documented in human patients (Gomez-Isla et al., 1996; Calhoun et al., 1998; de Toledo-Morrell et al., 2000; Du et al., 2001; Kordower et al., 2001; Ribe et al., 2005). However, little is known about AD-associated changes in EC astroglia. Post-mortem studies have revealed an increase in GFAP (glial fibrillary acidic protein) protein levels as well as in the number of GFAP-positive astrocytes within the EC, which seems to be associated with the Aβ load (Muramori et al., 1998; Porchet et al., 2003). Recently, we reported the concomitant occurrence of astroglial atrophy and astrogliosis in the HC of the transgenic mice model of AD. The atrophy appears as a generalized process, whereas astrogliosis was triggered by developing SPs and Aβ aggregates (Rodríguez et al., 2009b; Heneka et al., 2010; Olabarria et al., 2010; Verkhratsky et al., 2010; Rodríguez and Verkhratsky, 2011). In the present paper, we extended our analysis of AD-associated changes in astroglia to the EC.

MATERIALS AND METHODS

All animal procedures were carried out in accordance with the United Kingdom Animals (Scientific Procedures) Act of 1986 under license from the Home Office. All efforts were made to reduce the number of animals by following the 3R's.

Animal models

The generation of 3xTg-AD (triple transgenic mice of AD) mice has been well described (Oddo et al., 2003a, 2003b; Billings et al., 2005; Rodríguez et al., 2008; Rodríguez et al., 2009a, 2009b). The 3xTg-AD mice were derived from mixed 129/C57BL6 mice, which harbour APPswe, PS1M146V and TauP301L mutations, and the same spatiotemporal progression of amyloid and tau protein pathology in human AD. The non-Tg (non-transgenic) control mice were from the same strain and the same genetic background. All 3xTg-AD and non-Tg littermates were from homozygous breeders. Mice were grouped by gender and genotype, housed under controlled temperature and 12 h light/12 h dark cycles with ad libitum access to food and water.

Fixation and tissue processing

As previously described (Olabarria et al., 2010), male 3xTg-AD at 1, 3, 6, 9 and 12 months of age (n = 5, 4, 4, 5 and 5 respectively) and their age-corresponding non-Tg controls (n = 4, 4, 4, 5, 5 respectively) were anaesthetized with sodium pentobarbital (50 mg/kg) intraperitoneally. The brains were fixed by aortic arch perfusion of 3.75% acrolein (25 ml; TAAB, UK) in 2% (w/v) paraformaldehyde (Sigma, St. Louis, MO, U.S.A.) and 0.1 M PB (phosphate buffer) at pH 7.4, followed by 75 ml of 2% paraformaldehyde. Brains were removed, cut into 2–3 mm coronal slabs containing the EC, post-fixed in 2% paraformaldehyde for 24 h and sectioned at 40–50 μm with a vibrating microtome (VT1000S; Leica, Milton Keynes, U.K.). Free-floating sections in 0.1 M PB were collected and stored in a cryoprotectant solution containing 25% sucrose and 3.5% glycerol in 0.05 M PB at pH 7.4. Coronal sections at levels −2.30 mm/−3.88 mm [LEC (lateral entorhinal cortex)] posterior to Bregma were selected for immunohistochemistry according to the mouse brain atlas of Paxinos and Franklin (2004).

Antibodies

To detect and determine the changes in the astrocytic cytoskeleton in the EC, we used a monoclonal mouse antiserum against GFAP (anti-GFAP; Sigma–Aldrich; #G3893). For the identification of Aβ aggregation as well as the relation of astrocytic cytoskeleton alteration with Aβ, we used a polyclonal rabbit anti-GFAP serum (Sigma–Aldrich; #G9269) and a monoclonal mouse antiserum against amino acid residues 1–16 of Aβ, which reacts with abnormally processed isoforms and precursor form of Aβ [EFRHDS; anti-Aβ 6E10 (SIG-39320), Signet Laboratories, Dedham, MA, U.S.A.]. For the detection of NFTs, we used a monoclonal mouse antiserum against PHF (paired helical filament) tau protein, which recognizes phosphorylated Ser-202/Thr-205 of tau protein (Innogenetics, Zwijndrecht, Belgium). The immunolabelling pattern we obtained with this antibody is equivalent to that obtained previously in different brain regions (Oddo et al., 2003a). Positive and negative control immunohistochemistry was used to test non-specific labelling and/or cross-reaction between antisera derived from different host species, showing no immunoreactivity (data not shown). The specificity of these antisera was confirmed by immunohistochemistry and Western blotting in previous papers (Goedert 1995; Halliday et al., 1996; Rodríguez et al, 2008).

Immunocytochemistry

The procedure for immunocytochemistry was as described previously (Olabarria et al., 2010; Noristani et al., 2010). All sections from both non-Tg and 3xTg-AD groups at different ages were processed at the same time using precisely the same experimental conditions to minimize methodological variability. Sections were pretreated with 30% (v/v) methanol and 3% H2O2 in 0.1 M PB for 30 min and subsequently a 1% sodium borohydride (Sigma–Aldrich) solution for 30 min. After washing with PB profusely, sections were then rinsed with 0.1 M TS (Tizma-based saline; Sigma–Aldrich), followed by incubation in 0.5% BSA (Sigma–Aldrich) and 0.25% Triton X-100 (Sigma) for 30 min. The sections were incubated in 0.1% BSA in 0.1 M TS at pH 7.6 and 0.25% Triton X-100 containing the following antibodies: monoclonal mouse anti-GFAP (1:5000; Sigma), monoclonal mouse anti-Aβ (1:1000; Covance, Emeryville, CA, U.S.A.) or monoclonal mouse anti-PHF tau protein (1:1000; Innogenetics) at room temperature (RT) (20–25°C) for 48 h. The sections were rinsed with TS and incubated in biotinylated horse anti-mouse IgG (1:200; Vector Laboratories, Peterborough, U.K.) at RT for 1 h. After rinsing with TS for 30 min, sections were incubated with avidin–biotin peroxidase complex (Vector Laboratories). The peroxidase reaction was carried out by incubation with a solution containing 0.022% DAB (diaminobenzidine; Aldrich) or 0.003% H2O2, or the SG peroxidase substrate kit (Vector Laboratories) for 5 min. Sections were then dehydrated in ascending concentration of ethanol (50, 70, 80, 90, 95 and 100%) and subsequently xylene, and then permanently coverslipped with the use of Entellan (Merck).

For single fluorescent labelling, the sections were then incubated for 48 h at RT in the primary antibody solution as mentioned above. Sections were then rinsed with 0.1 M TS and incubated in secondary solution containing FITC-conjugated goat anti-mouse IgG (1:100; Jackson Immunoresearch, Baltimore Pike, PA, U.S.A.) for 1 h at RT.

For dual labelling, the sections were incubated for 48 h at RT in a primary antibody cocktail containing (i) monoclonal mouse anti-Aβ antibody (1:1000; Covance) and (ii) rabbit anti-GFAP (1:5000; Sigma) simultaneously. Sections were washed with 0.1 M TS and incubated in rhodamine [TRITC (tetramethylrhodamine β-isothiocyanate)]-conjugated goat anti-rabbit for the detection of GFAP, followed by rinsing with TS. Subsequently, the sections were incubated in FITC-conjugated goat anti-mouse IgG (Invitrogen, Paisley, U.K.) for the detection of Aβ. All the sections were mounted in an aqueous medium (Vectashield; Vector Laboratories).

Morphological analysis of the astrocytic cytoskeleton

GFAP-positive astrocytes (n = 30–35 in single fluorescent labelling experiments) throughout the layer of the LEC were imaged by using confocal microscopy (Leica SP5, Mannheim, Germany) with 0.2 μm z-step size. Parallel confocal planes were superimposed and Cell Analyst program (Chvatal et al., 2007) was used for analysis. Five digital filters (average 3×3, convolution, gauss 5×5, despeckle, simple objects removal) with a threshold of 50 were used to determine the surface and volume of the GFAP-positive astrocytic cytoskeleton. When analysing astroglial morphology in relation to Aβ plaques, all cells with somata within 50 μm from the plaque border were regarded as plaque associated, and cells with somata located more distantly (>50 μm) as cells not associated with plaques (Olabarria et al., 2010).

GFAP-IR (glial fibrillary acidic protein-immunoreactive) cell count in the EC

To determine the Nv (numerical density) of GFAP-IR astrocytes in the EC, we counted the number of GFAP-IR astrocytes throughout the layers of the whole LEC, an area of 435000 μm2 in coronal sections with 40 μm thickness in three or four representative non-consecutive sections. Confocal stack images were used for this purpose. GFAP-IR astrocytes were intensely labelled against dark background, which made them easy to identify with equal chances of being counted. The analysis was performed blindly with regard to mouse genotype.

Statistical analysis

Data are expressed as means±S.E.M. The paired or unpaired Student's t test was used to examine differences in the Nv, surface, volume and somata volume of GFAP-labelled cells between 3xTg-AD and non-Tg animals, using Graphpad Prism (GraphPad Software, La Jolla, CA, U.S.A.). P⩽0.05 was considered statistically significant.

RESULTS

GFAP-IR cells were widely distributed throughout the EC of both non-Tg and 3xTg-AD mice (Figures 2A–2F), with layers I and VI being the ones showing more GFAP-IR cells and stronger immunoreactivity (Figures 2A and 2B). GFAP-IR showed multiple branched processes extending in different directions from elongated cell bodies (Figures 3D–3G).

Figure 2. Comparison of GFAP-IR cell distribution and density in the EC of non-Tg and 3xTg-AD animals.

Figure 2

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Bright-field micrographs show the distribution of GFAP-IR astrocytes in the EC of non-Tg and 3xTg-AD animals (A and B respectively). Confocal imaging shows the organization of GFAP-IR astrocytes in the EC of non-Tg and 3xTg-AD animals at 1 month (C and D respectively) and 12 months (E and F respectively) at higher magnification. The histogram shows the Nv (number of cells per mm3) of GFAP-IR cells in the EC of 3xTg-AD and non-Tg controls (G). Results are means±S.E.M.

Figure 3. Comparison of astrocytic GFAP surface and volume in the whole EC of non-Tg and 3xTg-AD animals across ages.

Figure 3

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The histograms show a comparison of GFAP (A) surface, (B) volume and (C) body volume in the global EC at the age of 1, 3, 6, 9 and 12 months between 3xTg-AD and non-Tg animals. Results are means±S.E.M. (*P≤0.05 compared with the age-matched non-Tg control). Confocal micrographs show astrocytic atrophy in 3xTg-AD at 1 month (E) and 12 months (G) compared with the control animals (D and F).

Astrocytic cytoskeletal atrophy in 3xTg-AD mice

From 1 month of age, we observed morphological remodelling of EC astrocytes in 3xTg-AD mice compared with non-Tg animals. The astrocytes in 3xTg-AD animals had reduced primary branches (on average by 26%) originating from the soma and a markedly reduced presence of secondary processes extending from the primary branches (reduced by 30% on average), as well as distal ramifications (reduced by 45%; Figures 3D–3G). These changes indicate a morphological atrophy which was further confirmed by a significant decrease in both the surface and volume of GFAP profiles in the EC of 3xTg-AD animals when compared with non-Tg controls (Figures 3A and 3B). At younger ages (1 month), astrocytes of 3xTg-AD mice showed a significant decrease in GFAP surface when compared with the control. The surface area of GFAP-IR profiles was reduced by 48% (378.45±64.56 μm2 compared with 728.47±96.67 μm2; P = 0.017; Figure 3A). The volume of GFAP-IR cells in 3xTg-AD was reduced by 54% (115.38±25.82 μm3 compared with 252.94±32.73 μm3; P = 0.012; Figure 3B). This atrophic glial appearance was sustained through all ages up to 12 months (Figures 3A and 3B). This reduction was significant at 3 and 6 months of age; the surface area was decreased by 44 and 39% (378.56±64.53 μm2 compared with 680.20±53.70 μm2, P = 0.036; 354.68±67.74 μm2 compared with 581.26±70.13 μm2, P = 0.025 respectively; Figure 3A). The volume of GFAP-IR cells decreased by 42 and 42% respectively (130.25±25.82 μm3 compared with 224.32±18.80 μm3, P = 0.0490; 116.15±25.63 μm3 compared with 200.64±31.07 μm3, P = 0.025 respectively; Figure 3B). However, from 9 months of age onwards the degree of atrophic changes became somewhat less pronounced because of parallel atrophic changes developing in healthy aged controls. At 9 months of age, the surface and volume of astrocytes in 3x-Tg-AD animals were reduced, compared with the control, by 26% (391.04±30.75 μm2 compared with 529.47±48.21 μm2, P = 0.008) and 25% (130.92±12.40 μm3 compared with 174.71±15.41 μm3, P = 0.014) respectively (Figures 3A and 3B). Likewise, at 12 months of age the decrease in surface and volume was 33% (387.73±47.75 μm2 compared with 578.16±84.46 μm2; P = 0.021; Figure 3B) and 45% (130.73±14.93 μm3 compared with 200.13±25.18 μm3; P = 0.017) respectively (Figures 3A and 3B).

This generalized atrophy was also confirmed by a parallel and significant decrease in the somata volume of GFAP-IR astrocytes at a very early age (1 month) (41.63±7.43 μm3 compared with 71.69±7.68 μm3; P = 0.027; Figure 3C) when compared with control mice. However, at later ages, this decrease in somata volume persisted but became insignificant when compared with non-Tg due to a parallel decrease in non-Tg animals.

Layer-specific astrocytic atrophy during AD

We found a significant decrease in GFAP-IR cell surface areas in layers II, III and VI of 3xTg-AD animals when compared with controls from 1 month of age by 57% (323.57±53.89 μm2 compared with 769.28±180.91 μm2; P = 0.035), 45% (305.36±70.05 μm2 compared with 564.42±62.21 μm2; P = 0.031) and 56% (416.65±87.62 μm2 compared with 964.04±118.84 μm2; P = 0.007; Figure 4A) respectively. This decrease in the GFAP surface was also paralleled by a reduction in the cell volume in all layers: a reduction in volume of 66% in layer II (84.78±17.82 μm3 compared with 251.43±65.01 μm3; P = 0.028), 68% in layer III (59.57±16.16 μm3 compared with 187.70±26.64 μm3; P = 0.004) and 71% in layer VI (132.08±44.52 μm3 compared with 360.13±38.71 μm3; P = 0.0072; Figure 4B). However, we did not find any significant difference in the other layers, layers I and V.

Figure 4. Comparison of astrocytic GFAP EC surface and volume at different ages.

Figure 4

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The histograms show decreased GFAP surface (A, C, E) and volume (B, D, F) within specific layers between 3xTg-AD animals at the ages of 1, 6 and 12 months respectively. Results are means±S.E.M. (*P≤0.05; **P≤0.01 compared with the age-matched non-Tg control).

However, at middle age (6 months), these atrophic changes in surface and volume occurred only in layers II and V. The surface decreased by 38% (320.53±71.52 μm2 compared with 520.03±79.62 μm2; P = 0.021) and 41% (386.35±97.00 μm2 compared with 650.50±70.60 μm2; P = 0.004) in layers II and V respectively (Figure 4C); the volume decreased by 45% (93.74±24.85 μm3 compared with 169.19±38.39 μm3; P = 0.023) and 42% (130.43±37.92 μm3 compared with 224.85±34.16 μm3; P = 0.011) in layers II and V respectively (Figure 4D). However, no significant decline in either surface or volume was found in layers I, III and VI.

Finally, at later ages (12 months), the decrease in either surface or volume was restricted to layer VI but had a similar significance. 3xTg-AD animals showed a decrease in GFAP surface by 43% (418.81±53.84 μm2 compared with 739.91±56.20 μm2; P = 0.007) and in volume by 49% (149.03±23.85 μm3 compared with 290.03±29.20 μm3; P = 0.004; Figures 4E and 4F).

Astrocytic atrophy in the EC is not associated with loss of GFAP-IR astrocytes

The density of astrocytes in the EC and in different layers of EC of 3xTg-AD mice when compared with non-Tg mice was constant at all ages (Figure 2E). The distribution of GFAP-IR cells throughout the EC was also similar at all ages (Figure 2).

Rare association of astrocytes with Aβ plaques and absence of hypertrophic reaction

The presence of intraneuronal Aβ accumulation in EC is evident from 9 months of age, although plaques and extracellular aggregates are not present until 12 months of age (Figure 5). However, notwithstanding Aβ accumulation, GFAP-IR astrocytes rarely appear to be associated with Aβ-positive neurons, extracellular Aβ aggregates or SPs in the 3xTg-AD animals. All in all, less than 5% of astrocytes were located at a distance <50 μm to the SP. Most importantly, however, we failed to observe any signs of hypertrophy in EC astrocytes in 3xTg-AD animals at all ages; astroglial cells always demonstrated atrophic morphology.

Figure 5. Distribution and relationship of GFAP immunoreactive astrocytes and β-amyloid presence.

Figure 5

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Confocal images of dual labelling of GFAP (red) and Aβ (green) show that GFAP-IR astrocytes are distant from intracellular Aβ deposits (with a distance of 86 μm) at 12 months and distant from the Aβ plaques (with a distance of 125 μm) at 18 months. Arrowheads indicate astrocytes.

DISCUSSION

The EC is regarded as a funnel for cortico-hippocampal information transfer and integration, playing an essential role in cognition and memory (Kerr et al., 2007; Canto et al., 2008; Coutureau and Di Scala, 2009). In the present study, for the first time we present evidence indicating an early (from 1 month of age) atrophy of astrocytes in the EC of 3xTg-AD mice; this atrophy being sustained through more advanced ages (up to 12 months). This atrophic remodelling occurred in the superficial and deep layers at early and middle age (1–6 months), although at later ages (12 months) it remained only in the deeper layers. The morphological atrophy of astroglia is not accompanied by an astrocytic loss at all ages.

The generalized atrophy characterized by a major reduction in astrocytic primary branches and massive reduction in secondary and distal processes in the EC appears in very young 3xTg-AD animals (1 months old), which did not show yet any signs of AD pathology. This atrophic appearance remains in later ages (12 months), distinguished by developed Aβ plaques and NFTs, which are confirmed by the immunoreactivity of Aβ and phosphorylated tau protein (Supplementary Figure S1 at http://www.asnneuro.org/an/003/an003e071add.htm; Oddo et al., 2003b; Rodríguez et al., 2009b). Consistent reduction in the GFAP expression is in agreement with our previous observations of generalized atrophy of astrocytes in the HC, which similarly appear before the neuropathological marks (from 9 months) and are sustained in later ages (up to 18 months; Rodríguez et al., 2009b; Olabarria et al., 2010). Although some post-mortem studies have revealed hypertrophic astrocytes, characteristic of astrogliosis in the EC of AD human patients (Muramori et al., 1998; Porchet et al., 2003, Vanzani et al., 2005), this is only related to intralaminar astrocytes, since interlaminar astrocytes also showed disrupted processes and dynamic properties (Colombo et al., 2002). Furthermore, microarray analysis also showed a decrease in gene transcription of astrocytic cytoskeleton proteins in AD, implying a down-regulation of the astrocytic cytoskeleton (Simpson et al., 2011). At the same time, the density of GFAP-IR cells remains constant at all ages in both the control and 3xTg-AD. This indicates that neither aging nor AD pathology triggers cell loss. These data again correspond to our previous study and argue against the prominent astroglial proliferative response in the 3xTg-AD brain (Olabarria et al., 2010).

Astrocytic atrophy in the EC occurred very early, at 1 month of age. This is somewhat similar to the general observation that the AD pathology is manifested by Aβ accumulation, which begins in neocortex and rhinal cortices, including the EC, subsequently progressing to the HC and eventually appearing in all subcortical areas (Braak and Braak, 1997; Thal et al., 2000). The formation of neurofibrillary tangles initiates in the transentorhinal as well as entorhinal cortices, advancing to the HC through the perforant path and neighbouring cortical regions (Braak et al., 1999). The spatiotemporal occurrence of astroglial atrophy is therefore consistent with pathological hallmarks of AD, indicating that the EC is the region first affected by AD pathology. The evident changes in entorhinal astrocytes appear within layers II, III and VI at early age (1 month); layers II and V are affected at middle age (6 months), while they are restricted in layer VI at later ages (12 months). Nevertheless, it should be noted that there is no recovery of atrophic astrocytes in transgenic mice in the superficial layers at later ages but a decrease in GFAP in non-Tg controls, implying an aging effect on control animals (Figure 3).

Astroglia sustain multiple functions, including balance of neurotransmitters, release of trophic factors, metabolic support and extracellular ion buffering, all of which maintain brain physiology and support neuronal connectivity (Danbolt, 2001; Nedergaard et al., 2003; Wang and Bordey, 2008; Verkhratsky et al., 2010, 2011). In addition, astrocytes are able to sense synaptic activity, regulate synaptic plasticity and synchronize neuronal networks, thus being involved in conscience and cognitive processes (Araque et al., 1999; Fellin et al., 2004; Henneberger et al., 2010; Lalo et al., 2006, 2011). Finally, by virtue of astrogliosis, astrocytes form the innate brain defence system, localizing the lesions and assisting in pathological remodelling of the affected circuitry (Sofroniew, 2009). Early astroglial atrophy observed in EC may result in reduced astroglial coverage of synapses and thus may appear to be a key factor in altered synaptic connectivity (Rodríguez et al., 2009b; Verkhratsky et al., 2010). In consequence, the synaptic condition and/or activity may be affected, causing synaptic remodelling, altered synaptic connections and network activity. It is likely that this early astrocytic alteration leads to compromised EC output to other areas, especially the HC that receives innervation from both the superficial and deep layers of the EC (Figure 1). In fact, there is no significant neuronal loss in memory-associated areas, such as the EC and HC, in the 3xTg-AD animal model (Oddo et al., 2003a, 2003b; Rohn et al., 2008; Bittner et al., 2010). Nonetheless, loss of synapses and/or dendritic spines as well as compromised long-term potentiation have been detected in several brain regions, suggesting impaired synaptic connectivity and functions in this animal model (Oddo et al., 2003a; Bertoni-Freddari et al., 2008; Bittner et al., 2010; Noristani et al., 2011). Therefore the astrocytic atrophy in the EC may underlie synaptic pathology being the basis of cognitive and memory impairment at the early stages of the AD.

In contrast with the HC (Olabarria et al., 2010), arrival of Aβ depositions and SPs in the EC does not trigger astrolgiotic reaction at least from the morphological criteria. We failed to observe a close association of astrocytes with SPs; nor did we find any signs of astroglial hypertrophy. This peculiar indifference of EC astrocytes to the AD-specific lesion may underlie the particular vulnerability of the EC to the AD-like pathology and provide an explanation of why EC is the first brain region to be affected in the course of AD. Obviously, further studies are required to extend the findings from the AD animal model to human pathology.

Footnotes

This work was supported by an Alzheimer's Research Trust's Programme Grant [grant number ART/PG2004A/1 (to J.J.R. and A.V.)]; the Grant Agency of the Czech Republic [grant numbers GACR 309/09/1696 and GACR 304/11/0184 (to J.J.R.) and GACR 305/08/1381 and GACR 305/08/1384 (to A.V.)]; the Spanish Government, Plan Nacional de I+D+I 2008–2011 and ISCIII-Subdirección General de Evaluación y Fomento de la investigación [grant number PI10/02738 (to J.J.R. and A.V.)]; and the Government of the Basque Country grants [grant numbers AE-2010-1-28 and AEGV10/16 (to J.J.R.)].

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