Oxidative Stress during the Progression of <i>β</i>-Amyloid Pathology in the Neocortex of the Tg2576 Mouse Model of Alzheimer’s Disease

Porcellotti, Sara; Fanelli, Francesca; Fracassi, Anna; Sepe, Sara; Cecconi, Francesco; Bernardi, Cinzia; Cimini, AnnaMaria; Cerù, Maria Paola; Moreno, Sandra

doi:https://doi.org/10.1155/2015/967203

Oxidative Medicine and Cellular Longevity

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Research Article | Open Access

Volume 2015 | Article ID 967203 | https://doi.org/10.1155/2015/967203

Oxidative Stress during the Progression of β-Amyloid Pathology in the Neocortex of the Tg2576 Mouse Model of Alzheimer’s Disease

Sara Porcellotti,¹Francesca Fanelli,¹Anna Fracassi,¹Sara Sepe,^1,2Francesco Cecconi,³Cinzia Bernardi,⁴AnnaMaria Cimini,⁵Maria Paola Cerù,^1,5and Sandra Moreno¹

Academic Editor: Ryuichi Morishita

Received30 Dec 2014

Revised26 Mar 2015

Accepted27 Mar 2015

Published20 Apr 2015

Abstract

Alzheimer’s disease (AD) is the most common form of dementia, characterized by progressive neurodegeneration. Pathogenetic mechanisms, triggered by β-amyloid (Aβ) accumulation, include oxidative stress, derived from energy homeostasis deregulation and involving mitochondria and peroxisomes. We here addressed the oxidative stress status and the elicited cellular response at the onset and during the progression of Aβ pathology, studying the neocortex of Tg2576 model of AD. Age-dependent changes of oxidative damage markers, antioxidant enzymes, and related transcription factors were analysed in relation to the distribution of Aβ peptide and oligomers, by a combined molecular/morphological approach. Nucleic acid oxidative damage, accompanied by defective antioxidant defences, and decreased PGC1α expression are already detected in 3-month-old Tg2576 neurons. Conversely, PPARα is increased in these cells, with its cytoplasmic localization suggesting nongenomic, anti-inflammatory actions. At 6 months, when intracellular Aβ accumulates, PMP70 is downregulated, indicating impairment of fatty acids peroxisomal translocation and their consequent harmful accumulation. In 9-month-old Tg2576 neocortex, Aβ oligomers and acrolein deposition correlate with GFAP, GPX1, and PMP70 increases, supporting a compensatory response, involving astroglial peroxisomes. At severe pathological stages, when senile plaques disrupt cortical cytoarchitecture, antioxidant capacity is gradually lost. Overall, our data suggest early therapeutic intervention in AD, also targeting peroxisomes.

1. Introduction

Alzheimer’s disease (AD) is the most common form of dementia, characterized by progressive neurodegeneration, particularly affecting cortical and hippocampal brain regions [1]. Histopathological features of AD are senile plaques, composed of β-amyloid (Aβ) peptide polymers, and intracellular neurofibrillary tangles, formed by hyperphosphorylated Tau protein. Aβ peptide is produced by neurons through the processing of APP and has the propensity to aggregate in oligomers, which are more neurotoxic than Aβ plaques themselves [2].

Two forms of the disease are classified, according to the age of manifestation of the disease, namely, early onset AD (EOAD) and late onset AD (LOAD). The former has been associated with the presence of mutations to the genes encoding for amyloid precursor protein (APP), presenilin 1 and presenilin 2 (PSEN1 and PSEN2) [3]. Based on these genetic studies, several animal models have been so far generated [4], among which the Tg2576 mouse strain harboring the human APPswe mutant allele linked to familial Alzheimer’s disease, is one of the most widely used [5]. Although these mice lack neurofibrillary tangles and substantial neuronal loss, they develop early synaptic deficits and late neuropathological features, including amyloid plaques and dystrophic neurites [6]. Therefore, accumulation of Aβ peptide, leading to Aβ pathology, is responsible for age-related memory decline in this model [7, 8], thus reproducing rather faithfully the slow progression of human clinical symptoms and allowing dissecting the mechanisms underlying the onset and progression of disease [6–11].

Growing evidence has demonstrated that oxidative stress is an important factor contributing to the initiation and progression of AD [12]. Reactive oxygen species (ROS) production in AD derives from deregulation of energy homeostasis, hence involving mitochondria and peroxisomes, cellular compartments importantly participating in ROS and lipid metabolism [13, 14].

Imbalance in the redox status activates an array of cell response mechanisms, including expression and activation of nuclear receptors and their cofactors regulating energy metabolism and antioxidant defences [15]. Among these, peroxisome proliferator activated receptors (PPARs), comprising three isotypes (α, β, and γ), regulate both mitochondrial and peroxisomal biogenesis and functions [16, 17]. Importantly, beneficial effects of PPAR agonists on AD-related neurodegeneration are reported by several groups [18, 19], strongly suggesting that therapeutic strategies targeting these molecules are promising in preventing AD onset and progression. Among PPAR coactivators, PGC1α is the most extensively studied, for its wide array of functions, including glucose metabolism, fatty acid oxidation, ROS scavenging, and mitochondrial/peroxisomal biogenesis and functioning [20, 21].

In previous works, we reported variations of antioxidant and lipid metabolizing enzymes at the onset [22] and during the progression [10] of Aβ pathology, in Tg2576 (Tg) mice. The former study focused on early changes in neocortical and hippocampal tissues; the latter emphasized the age-dependent role of peroxisomes and PPARα in the hippocampus.

The present work extends the analysis of oxidative stress and the elicited cellular response to the neocortex of Tg mice, aging 3, 6, 9, 12, and 18 months, as compared to wild type (WT) littermates. The variations of oxidative damage markers, redox status sensors, and antioxidant and peroxisomal proteins were studied in relation to the accumulation of neurotoxic Aβ peptide and oligomers.

2. Materials and Methods

2.1. Animals

Heterozygous female Tg2576 mice [5] and WT littermates were used for all experiments. Male mice (C57B6 × SJL), hemizygous for human APP695 carrying the double mutation K670N and M671L (FADSwedish mutation), were purchased from Taconic Farms, Inc. (Germantown, NY, USA). The Tg colony is maintained and the genotyping is performed as previously described [22]. For all analyses, Tg and WT female mice of 3, 6, 9, 12, and 18 months of age were used.

Experiments were performed in accordance with the European Community’s Council Directive 86/609/EEC. Formal approval of these experiments was obtained from the Italian Ministry of Health (D.L.vo 116/92; Prot. number 155-VI-1.1). All efforts were made to minimize the number of animals used and their suffering.

2.2. Molecular Analyses

Six animals from each age group (three Tg and three WT) were killed by cervical dislocation, brains were rapidly excised on an ice-cold plate, and cortices were dissected out.

Cortical Tissue Homogenate Preparation and Protein Extraction. A lysis buffer (320 mM sucrose, 50 mM NaCl, 50 mM Tris–HCl, pH 7.5, 1% Triton X-100, 0.5 mM sodium orthovanadate, 5 mM β-glycerophosphate, and 1% protease inhibitor) was used to homogenate cortical tissue, incubating the samples on ice for 30 min. Homogenates were centrifuged at 13,000 rpm for 10 min at 4°C. The total protein content of the resulting supernatant was determined using a spectrophotometric assay, according to the method described by Bradford [23]. Samples were then diluted 3 : 4 in 200 mM Tris–HCl, pH 6.8, containing 40% glycerol, 20% β-mercaptoethanol, 4% sodium dodecyl sulphate (SDS), and bromophenol blue.

2.3. Western Blotting (WB)

In WB experiments, performed as previously described [22], membranes were probed at 4°C overnight with either of the following primary antibodies: 1 : 200 rabbit polyclonal antiglial fibrillary acidic protein (anti-GFAP, Sigma-Aldrich, St. Louis, MO, USA); 1 : 1000 rabbit polyclonal anti-SOD1 (Abcam, Cambridge Science Park, Cambridge, UK); 1 : 10000 anti-SOD2 (Abcam); 1 : 3000 rabbit polyclonal anti-GPX1 (Abnova, Taipei City, Taiwan); 1 : 2000 rabbit polyclonal anti-CAT (Rockland, Gilbertsville, PA, USA); 1 : 1000 rabbit polyclonal anti-PMP70 (Sigma-Aldrich); 1 : 10000 rabbit polyclonal anti-Pex14p (generous gift from Professor R. Erdmann, Ruhr University Bochum, Bochum, Germany); 1 : 1000 rabbit polyclonal anti-AOX (generous gift from Professor A. Völkl, University of Heidelberg, Heidelberg, Germany); 1 : 1000 rabbit polyclonal anti-THL (generous gift of Professor P. Van Veldhoven, Katholieke Universiteit Leuven, Leuven, Belgium); and 1 : 3000 mouse monoclonal anti-β-actin (Sigma-Aldrich). Membranes were then incubated with 1 : 2000 HRP-conjugated goat anti-rabbit or anti-mouse IgG secondary antibodies (Santa Cruz Biotechnology, Santa Cruz, CA, USA) in blocking solution, for 1 h at 4°C. Immunoreactive bands were visualized by a chemiluminescence detection kit (ECL Plus Western Blotting Detection Reagents, Amersham GE Healthcare, Little Chalfont, UK). The relative densities of immunoreactivity were determined by densitometry using the software ImageJ (NIH, Bethesda, MD, USA) and normalized with respect to β-actin. Data are mean of five different experiments.

2.4. Statistical Analyses

Statistical evaluation of WB experiments was performed using GraphPad Prism 4 software. For comparison between genotypes and among different ages, statistical analysis of WB densitometric values was accomplished using two-way analysis of variance (ANOVA) followed by the Bonferroni test to detect significant differences between groups. Means from independent experiments were then expressed as means ± SD. For all statistical analyses, was considered as statistically significant.

2.5. Morphological Analyses

2.5.1. Brain Tissue Preparation and Sectioning for Light and Confocal Microscopy

For each age considered, 3 Tg mice and 3 WT littermates were deeply anesthetized with urethane (1 g/kg body weight, injected i.p.), before rapid killing by transcardial perfusion with the fixative solution, as previously described [22]. Brains were dissected out, sagittally cut along the midline, and paraffin-embedded.

Serial, 5 μm thick sagittal sections from each Tg and WT brain sample were obtained by a rotary microtome, till exhaustion of the specimens. For each marker to be analyzed, five sections from each brain sample were processed.

2.5.2. Congo Red Staining

Deparaffinized sections were treated with hematoxylin for 15 minutes, immersed in a 0.5% acid ethanol solution and then in a Congo Red solution (composed of 2.5% NaCl, 50% ethanol solution, 0.01% KOH solution, and 0.2% Congo Red). Finally, sections were dehydrated and mounted with Eukitt. Slides were observed in an Olympus BX 51 microscope, under polarized light, to detect amyloid plaques for their birefringence. All the stained sections were extensively analysed and representative electronic images were captured by a Leica DFC 420 camera, using a Leica Application Suite system, and composed in an Adobe Photoshop CS5 format.

2.5.3. Immunohistochemistry (IHC)

For light microscopic immunolocalization, deparaffinized sections were processed as previously described [22]. The following primary antibodies were used: 1 : 100 mouse monoclonal anti-NeuN (Chemicon, Temecula, CA, USA); 1 : 300 rabbit polyclonal anti-GFAP (Dako, Glostrup, Denmark); 1 : 100 mouse monoclonal anti-Aβ (Synaptic Systems, Gottingen, Germany); 1 : 100 mouse monoclonal anti-oligo-pGlu Aβ (Synaptic Systems); 1 : 100 mouse monoclonal anti-Iba1 (Abcam); 1 : 500 mouse monoclonal anti-8-hydroxy(deoxy)guanosine (8-OHG) (QED Bioscience Inc., San Diego, CA, USA); 1 : 500 rabbit polyclonal anti-acrolein (generous gift from Professor K. Uchida, Nagoya University, Nagoya, Japan); 1 : 200 rabbit polyclonal anti-PPARα (ABR Affinity BioReagents, Golden, CO, USA); 1 : 50 mouse monoclonal anti-PGC1α (Calbiochem, Darmstadt, Germany); 1 : 100 rabbit polyclonal anti-SOD1 and 1 : 1000 anti-SOD2; 1 : 100 rabbit polyclonal anti-GPX1; and 1 : 200 rabbit polyclonal anti-PMP70. In control sections, the primary antibody was omitted. Biotinylated goat anti-rabbit or anti-mouse IgG (Vector Laboratories, Burlingame, CA, USA) were used as secondary antibodies and immunocomplexes were visualized, as previously reported [22]. Slides were dehydrated and mounted and then observed under an Olympus BX 51 microscope, equipped with a Leica DFC 420 camera. All immunoreacted sections were extensively analysed and representative electronic images were captured by a Leica Application Suite system and composed in an Adobe Photoshop CS5 format.

2.5.4. Immunofluorescence (IF)

For double immunofluorescence, deparaffinized sections from 3-month-old Tg brains were incubated with a mixture of 1 : 1000 anti-SOD2 and 1 : 500 anti-8-OHG, overnight at 4°C. Slides were thoroughly rinsed with PBS and then incubated for 1 h at RT with a mixture of 1 : 500 Chromeo 488-conjugated goat anti-rabbit IgG and 1 : 500 Chromeo 555-conjugated goat anti-mouse IgG (both from Invitrogen, Life Technologies Italia, Monza, Italy). All antibodies were diluted in PBS containing 4% BSA. Controls were performed by omitting the primary antibodies. Slides were mounted with Vectashield (Vector) and observed in a Leica TCS SP5 confocal microscope. Representative images, captured by a Leica Application Suite system, were composed in an Adobe Photoshop CS5 format.

2.5.5. Electron Microscopy

For the ages of 3, 6, and 9 months, one Tg mouse and one WT littermate were anesthetized and perfused, as described for light microscopy. Brains were dissected out and sagittally cut by a vibratome, obtaining 100 μm thick sections, to be processed for ultrastructural studies. Osmium postfixation, dehydration, and Epon flat-embedding were performed as previously described [22]. Select neocortical fields of resin-embedded sections, identified in a light microscope, were remounted on Epon blanks and further sectioned on a Reichert Ultracut S ultramicrotome. Ultrathin sections were briefly contrasted with uranyl acetate and observed in a Philips CM120 electron microscope equipped with a Philips Megaview III camera. Representative images were captured by AnalySys 2.0 software and composed in Adobe Photoshop CS5 format.

3. Results

3.1. Neural Cell Markers and Amyloid Deposits

To analyse cortical cytoarchitecture, the localization of the neuronal marker NeuN and the astroglial marker GFAP was studied by IHC (Figure 1).

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Figure 1

NeuN and GFAP expression in the neocortex of WT and Tg mice. (a) NeuN IHC localization in the neocortex of 3-, 6-, 9-, 12-, and 18-month-old WT and Tg mice. Arrows indicate amyloid plaques in 12- and 18-month-old mice. Scale bars, 40 μm. (b) Upper picture, GFAP WB densitometric analysis on neocortex protein extracts of 3-, 6-, 9-, 12-, and 18-month-old mice. Values are expressed as mean ± SD. ; . (b) Lower pictures, GFAP IHC distribution in 6-, 9-, 12-, and 18-month-old WT and Tg neocortex. Scale bars, 60 μm.

Alterations in the distribution of NeuN positive cells are only observed in Tg at late stages (12 and 18 months), when the overall layering is disrupted by the presence of large and progressively more numerous amyloid plaques. These deposits, found throughout the layers of the neocortex, are totally devoid of NeuN positive cells (Figures 1 and 2).

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(b)

Expression of GFAP, revealed by IHC and WB, is unchanged until 9 months, while a sustained increase in immunopositivity in Tg neocortex is detected thereafter (Figure 1). At 18 months of age, numerous hypertrophic astrocytes are found throughout the layers and, particularly, around senile plaques (Figures 1 and 2). Similar localization is shown by Iba1-positive microglia (Figure 2).

Senile plaques were recognised by Congo Red staining, using a polarizing filter (Figure 2). Small birefringent amyloid deposits are first detected in 9-month-old Tg neocortex. Their size and number progressively increase during aging, leading to cortical cytoarchitecture derangement.

Since Aβ, particularly in its oligomeric form, is considered the primary culprit of AD pathology [2], we studied the distribution of Aβ peptides and respective oligomers by IHC (Figure 3). The antibody to Aβ, recognising 1–38, 1–40, and 1–42 Aβ peptides, reveals no difference between WT and Tg at 3 months (not shown). A stronger immunoreactivity of Tg neurons, compared to WT, is instead observed starting from 6 months of age (Figure 3(a)). At later stages, Aβ accumulates extracellularly, especially within senile plaques.

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Figure 3

Amyloid deposits in WT and Tg neocortex. (a) Aβ IHC in 6-, 9-, and 18-month-old WT and Tg neocortex. A stronger staining is consistently present in Tg neurons, compared to WT. At late stages, Aβ accumulates within senile plaques. Scale bars, 40 μm. (b) Immunolocalization of anti-oligo-pyroGlu Aβ, revealing low molecular weight oligomers. The reaction product accumulates in Tg neocortex starting from 9 months and is observed both intra- and extracellularly, particularly inside the plaques. Scale bars, 40 μm.

Low molecular weight oligomers were immunolocalized by anti-oligo-pGlu Aβ, a truncated and pyroglutamate-modified form of Aβ, composing the central nucleus of plaques on which all other native Aβs aggregate [24]. Immunostaining accumulates in Tg neocortex starting from 9 months of age and is observed both intra- and extracellularly, particularly inside the plaques (Figure 3(b)).

3.2. Ultrastructural Analysis

Ultrastructural analysis performed on the neocortex of 3-, 6-, and 9-month-old animals shows genotype- and age-related differences (Figure 4). While 3-month-old samples, irrespective of the genotype, show normal ultrastructural features in both nuclear and cytoplasmic compartments, at 6 and 9 months this morphology is only conserved in WT neocortex (Figure 4(a)). By contrast, mild-to-severe lesions are detected in Tg neurons as a function of age, starting from 6 months (Figure 4(b)). Mitochondria are probably the most profoundly affected organelles, in that their outer and inner membranes appear irregularly arranged, with disrupted cristae and vacuolization. Abnormally dilated Golgi complex, accompanied by cisternae fragmentation, is also readily identified in Tg cells. Interestingly, in 9-month-old Tg neocortex, the occurrence of dense bodies is a frequent finding.

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Figure 4

Ultrastructural analyses of WT and Tg neocortex. (a) WT neocortical neurons from 3-, 6-, and 9-month-old animals. Regular ultrastructural features of the nuclear compartment (N) and cytoplasmic organelles (m, mitochondrion; er, endoplasmic reticulum; g, Golgi complex) are observed at all ages. (b) Tg neocortical neurons showing progressive damage, starting from 6 months of age. Mitochondrial (m) abnormalities include outer and inner membrane derangement, with disrupted cristae and vacuolization. Abnormally dilated Golgi complex (g), cisternae fragmentation (arrowheads), and numerous dense bodies (arrows) are also readily identified in 9-month-old Tg neocortical neurons.

3.3. Oxidative Stress Markers: 8-OHG and Acrolein

In view of the central role played by oxidative stress in AD and of the specific involvement of Aβ in ROS generation, we searched for oxidatively modified macromolecules. To this aim, the occurrence of 8-OHG and acrolein, as markers of oxidative damage to nucleic acids and lipids, respectively, was investigated by IHC (Figure 5).

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Figure 5

Expression of oxidative damage markers in WT and Tg neocortex. (a) 8-OHG IHC in 3-, 9-, and 18-month-old WT and Tg neocortex. Prominent cytoplasmic staining in Tg neurons is observed throughout the ages. Scale bars, 30 μm. (b) Acrolein IHC showing higher levels in Tg than in WT neurons, starting from the age of 9 months. Scale bars, 30 μm. (c) Double immunofluorescence of 8-OHG (red) in combination with SOD2 (green) in the neocortex of 3-month-old Tg mice, showing partial colocalization of both markers, thus indicating mitochondrial DNA oxidative modifications. Scale bars, 30 μm.

Age- and genotype-dependent alterations are detected for both markers. In particular, 8-OHG immunoreactivity levels are consistently higher in Tg, compared to WT, starting from 3 months. At 18 months, Tg neocortical plaques appear surrounded by 8-OHG-immunoreactive neuronal and glial cells, being negative themselves. Immunostaining is mainly localized to the cytoplasm, indicating modifications to mitochondrial nucleic acids and cytosolic RNA. Indeed, double IF in 3-month-old Tg neocortex demonstrates partial colocalization of the mitochondrial marker SOD2 with 8-OHG (Figure 5(c)). Interestingly, neurons expressing the highest levels of the antioxidant enzyme show relatively faint staining for the oxidative damage marker.

Acrolein, the most reactive aldehyde produced by lipid peroxidation, is consistently found in Tg neocortex at higher concentrations than in WT starting from 9 months (Figure 5). Senile plaques appear devoid of acrolein, but positive cells are found in their close proximity.

3.4. Transcriptional Regulators: PPARα and PGC1α

The expression and distribution of the oxidative stress sensors PPARα and PGC1α were investigated by IHC, at the onset and during the progression of Aβ pathology, as compared to normal brain aging.

Extensive analysis of PPARα immunoreacted sections (Figure 6(a)) revealed more intense positivity in Tg neocortex than in WT at 3 months, which however decreased thereafter, becoming fainter than in WT at 18 months. Interestingly, immunostaining, especially high in pyramidal cells (according to [25]), shows a somewhat different localization depending on the age and genotype. While in WT neocortex it is first (3 months) observed in the nucleus, progressively shifting to the cytoplasm, in Tg it appears predominantly cytoplasmic since the earliest stage.

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Differently from PPARα, PGC1α immunoreactivity at 3 months is lower in Tg than in WT neocortex (Figure 6(b)). Even though age-related increases are detected in both conditions, this genotype-based difference is maintained throughout the examined period and particularly apparent at 18 months. Similarly to PPARα, amyloid plaques are themselves PGC1α negative, while being surrounded by immunopositive cells.

3.5. Antioxidant Enzymes: SOD1, SOD2, and GPX1

The expression of ROS-scavenging enzymes was studied in WT and Tg neocortex by morphological and biochemical techniques.

SOD1 and SOD2 show early (3 months) downregulation in Tg neocortex, as demonstrated by both WB and IHC (Figure 7). No significant genotype-based differences are then detected at 6 and 9 months of age, while, at 12 months, higher expression levels in Tg than in WT neocortex are observed. This pattern reverts in 18-month-old neocortex, when Tg values are lower than WT ones. Concerning SOD2, remarkably strong immunoreactivity is detected in selected cortical neurons and in glial cells surrounding amyloid plaques.

Figure 7

SOD1 and SOD2 protein levels and distribution in WT and Tg neocortex. (a) Densitometric values of SOD1 WB of protein extracts from 3-, 6-, 9-, 12-, and 18-month-old WT and Tg neocortex. Data are expressed as mean ± SD. ; . (b) SOD1 IHC in WT and Tg neocortex. Higher expression levels in Tg than in WT neurons are found at 12 months, while the opposite is true for 18 months. Scale bars, 40 μm. (c) Densitometric values of SOD2 WB of protein extracts from 3-, 6-, 9-, 12-, and 18-month-old WT and Tg neocortex. Data are expressed as mean ± SD. ; ; . (d) SOD2 IHC in WT and Tg neocortex. Relatively low immunoreactivity levels in Tg neurons are found at 3 and 18 months, while at 12 months SOD2 expression is induced in Tg. Note striking immunostaining in glial cells surrounding and infiltrating amyloid plaques. Scale bars, 40 μm.

In both genotypes, GPX1 shows an age-related pattern characterized by progressive increase of protein levels from youth to maturity, followed by a decrease to minimal values in senescence (Figure 8). This pattern appears exacerbated in Tg neocortex, where the protein is downregulated with respect to WT at 3 months, overexpressed at 9 months, and again downregulated at 18 months, when immunostaining is almost exclusively concentrated at the senile plaques.

Figure 8

GPX1 expression and distribution in WT and Tg neocortex. GPX1 shows a strongly age- and genotype-related IHC pattern (a) consistent with WB densitometric data (b). Higher expression levels at 9 months and lower levels at 3 and 18 months are detected in Tg neocortex, as compared to WT. Values are expressed as mean ± SD. ; ; . The higher magnification micrograph (c) shows elevated immunoreactivity in glial cells surrounding and infiltrating an amyloid plaque of 18-month-old Tg neocortex. Scale bars, 40 μm.

3.6. Peroxisomal Proteins

Data obtained by WB and IHC on peroxisomal proteins are reported in Figure 9. While no age- or genotype-based differences of protein levels are detected for CAT, Pex14p, AOX, or THL, significant variations are observed for PMP70. This protein, involved in the transport of long and methyl-branched acyl-CoA esthers [26, 27] across the peroxisomal membrane, is highly expressed at 3 months in both genotypes and significantly downregulated at 6 months, particularly in the Tg neocortex, where the protein is almost reduced by half. A novel increase is observed in 9-month-old Tg, and these levels are maintained thereafter.

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Figure 9

Peroxisomal protein levels and distribution in the neocortex of WT and Tg mice. PMP70 expression showing downregulation at 6 months, as assessed by WB densitometry (a) and IHC distribution (b). Enhancement of PMP70 expression is observed in 9-month-old Tg neurons. Scale bars, 40 μm. (c) Densitometric analyses of WB for CAT, Pex14p, AOX, and THL performed on neocortical protein extracts from 3-, 6-, 9-, 12-, and 18-month-old mice. Significant downregulation of CAT in 6-month-old Tg neocortex is detected. Values are expressed as mean ± SD. ; ; .

4. Discussion

The aim of this work was to study age-dependent expression of some key biochemical markers of AD, with an emphasis on oxidative stress and antioxidant enzymatic response. We focused on the neocortex, as one of the most profoundly affected brain regions [1]. As a suitable model for this purpose and consistent with our previous investigations [9, 10, 22, 28], we chose the Tg2576 mouse model [5], which, differently from other models, displays a slowly progressive Aβ pathology. This offers the unique opportunity to study even subtle age-dependent alterations and, more importantly, to identify early biomarkers of the pathology and dissect the molecular mechanisms underlying the first symptoms [9, 22, 29–31]. In view of the greater amyloid load found in females of this specific transgenic model, we chose this gender [32].

In the present work, by comparing Tg animals with their WT littermates, we were able to detect early alterations of pathways related to homeostasis of cellular redox status. Indeed, reduced levels of the antioxidant enzymes GPX1, SOD1, and SOD2 are found in 3-month-old Tg neocortex. Moreover, the bioenergy sensor PGC1α, major regulator of their expression [33], shows low immunoreactivity levels in 3-month-old Tg neocortex. The role of this coactivator in AD is emphasized by reports on reduced levels of PGC1α in human patients and by the finding that PGC1α overexpression in Tg2576 primary neurons decreases Aβ levels [20]. Thus, our observations further support the concept that oxidative stress is a primary culprit in AD pathogenesis [34–36], in overall agreement with our previous study on the hippocampus [10]. However, it is worth mentioning that 3-month-old Tg neocortex shows an opposite SOD2 pattern, with respect to the hippocampus. Tentative explanation for this behavior could refer to differences in AD-associated changes in energy metabolism and in the elicited response in the two regions [22, 37]. Notwithstanding molecular alterations, we failed to detect any morphological change at the ultrastructural level in Tg neocortical neurons at this early stage.

As a likely consequence of decreased antioxidant defences, oxidatively modified nucleic acids are already detected in 3-month-old Tg neurons, particularly in the cytoplasm. Double IF, showing partial colocalization of 8-OHG with the mitochondrial marker SOD2, demonstrates early oxidative damage to mitochondrial nucleic acids, confirming that early redox cellular alterations in Aβ pathology involve mitochondrial dysfunction. Interestingly, cortical neurons appear heterogeneous in their immunoreactivity to SOD2, showing an inverse correlation between the abundance of the antioxidant enzyme and that of the oxidative damage marker, in agreement with the neuroprotective role of SOD2 [38–41].

In relation to these alterations, we studied the nuclear receptor PPARα, whose role in modulating cellular redox status and repressing inflammatory signaling pathways has long been established [42]. Growing evidence indicates neuroprotective action of PPARα agonists in Aβ pathology, even though the precise molecular mechanisms underlying such effects are yet to be deciphered [19, 43–45]. Our present results, in agreement with those previously reported for the hippocampal formation [10], show that PPARα is more abundant in 3-month-old Tg neocortex than in WT. This enhanced expression might represent the response to early redox unbalance. Intriguingly, the predominantly cytoplasmic immunostaining found in Tg neurons could reflect a nongenomic action, that is, tethering or squelching, leading to inhibition of inflammatory gene expression [16], albeit not excluding other still unknown functions of cytosolic PPARα. On the other hand, transcriptional activity of PPARα should be excluded, in view of our data on peroxisomal proteins. Indeed, expression of PMP70, Pex14, AOX, THL, and CAT, all encoded by PPRE-containing genes, is unchanged in 3-month-old Tg neocortices, compared to WT. At variance, in the hippocampal formation, PPARα mostly localized to the nuclear compartment, consistent with a genomic role of the transcription factor in upregulating its target genes PMP70, AOX, and CAT [10]. These differences may reflect region-specificity in terms of cell types relative abundance (astroglial versus neuronal), neuronal subtype diversity, and metabolic features involving energy metabolism [22, 37, 46].

Concerning peroxisomes, the decrease of PMP70 observed at 6 months, in the absence of alterations to other peroxisomal markers, could indicate that metabolic changes, rather than numerical reduction, of these organelles occur during physiological brain maturation. Consistent with our previous observation in the hippocampus [10], this decrease is exacerbated in Tg neocortex, demonstrating peroxisomal dysfunction consequent to Aβ-induced ROS overproduction. This condition may lead to cytosolic accumulation of long-chain unsaturated, dicarboxylic, and methyl-branched fatty acids, preferential substrates for PMP70-mediated transport [26, 27]. Among these molecules, phytanic and pristanic acids display a cytotoxic activity on brain cells, involving mitochondrial depolarization and ROS production, as demonstrated in different neural cell types and brain regions, including the neocortex [47, 48]. However, to our knowledge, information about levels of either phytanic or pristanic acid in AD patients or animal models is presently lacking. While the observed alterations to peroxisomes may participate in the disease progression, the origin of the alterations themselves might be ascribed to the direct neurotoxic action of Aβ peptide, which indeed is known to affect peroxisomal biogenesis and function [14, 49, 50]. Noteworthy, the age of 6 months is hallmarked by intracellular Aβ accumulation in Tg neocortex, undetectable at earlier stages. These data confirm and extend previous observations on the Tg2576 mouse model [5, 6], while suggesting early involvement of peroxisomal fatty acid dysmetabolism, leading to enhanced lipid peroxidation. Accordingly, and in agreement with Praticò and collaborators [51], our data demonstrate high immunoreactivity levels to acrolein in both the nucleus and the cytoplasm of 9-month-old Tg neurons. This byproduct of lipid peroxidation is the most reactive among others, inhibiting mitochondrial activity and decreasing glutathione levels [52]. Thus, acrolein has to be considered not only a lipid peroxidation marker, but also an initiator of oxidative stress in AD.

The above-mentioned age of 9 months seems crucial in the exacerbation of Aβ pathology. Ultrastructural analyses of neocortical neurons at this age demonstrate profound alterations to the cytoplasmic compartment. These abnormalities, which were milder at 6 months, mainly involve mitochondria and Golgi complex, consistent with electron microscopic observations on human tissue [53]. More specifically, mitochondria display deranged cristae and vacuolization, while Golgi complex shows dilated and fragmented cisternae, surrounded by numerous dense bodies. These morphological findings well correlate with the progression of Aβ pathology, witnessed by our IHC results showing increase in Aβ peptides concentration and first detection of oligomers, both intra- and extracellularly. Concomitantly, Congo Red staining reveals sporadic small senile plaques. Thus, our findings, in overall agreement with other authors [5, 6, 54], indicate an earlier appearance of histopathological signs in the neocortex than in the hippocampus [10]. Extracellular accumulation of Aβ induces astroglial activation, which in our samples is indeed revealed by enhanced GFAP immunoreactivity in 9-month-old Tg neocortex. Interestingly, at the same age, we show increased levels of GPX1, suggesting an adaptive response to Aβ-mediated H₂O₂ overproduction, also involving astroglia [55]. In 9-month-old Tg neocortex, similarly to what was observed in the hippocampus [10], we found increased PMP70 immunoreactivity, which also could be contributed by astroglia, taking into account the abundance of peroxisomes characterizing these cells [56, 57]. Thus, considering the relevant functions of these organelles in energy metabolism, with special reference to gluconeogenesis and to both inter- and intracellular lactate shuttling [58, 59], the increase in the fatty acid transporter PMP70 could be interpreted as an adaptive response of cortical astroglial peroxisomes to glucose hypometabolism, occurring early in AD [60].

At advanced Aβ pathology stages, oxidative stress exacerbates. At 12 months, expression levels of both SOD1 and SOD2 are higher in Tg than in WT, suggesting a compensatory response against superoxide-mediated damage. Accordingly, clinical findings revealed an upregulation of antioxidant enzymes in AD progression [41]. This response appears not to be triggered in the hippocampal formation, where SODs were both downregulated in 12-month-old Tg mice, with respect to their WT counterparts [10]. It is conceivable that the greater diversity in terms of neuronal subtypes in the cortical tissue may account for these region-based differences. This interpretation is supported by IHC data, showing, particularly for SOD2, strongly immunoreactive neurons, intermingled with faintly stained ones. While superoxide anions may therefore be efficiently detoxified in Tg neocortex, H₂O₂ (also produced by SOD activity) is unlikely to be concomitantly removed, since GPX1 and CAT levels are not increased. The progressively aggravating oxidative stress may contribute Aβ deposition and inflammation [61], leading to distortion of cortical cytoarchitecture, with abnormal neuronal layering and deposition of large senile plaques, which are surrounded by activated astrocytes (see NeuN and GFAP IHC). Concerning the biological significance of astrogliosis in AD, a dual role has been proposed, an early, beneficial one consisting of neuroprotective/metabolic support, as we propose to occur at the age of 9 months, and a late, detrimental one leading to inhibition of neurogenesis, parenchymal scarring, and self-perpetuating inflammation [62]. Indeed, onset of inflammatory processes is thought to occur late in the pathology [63–65].

Our data on 18-month-old neocortex demonstrate decreased capacity to respond to oxidative stress, since both redox status sensors and ROS-scavenging enzymes are overall reduced in Tg. Differently, aged WT mouse brain copes with oxidative stress by upregulating PPARα, PGC1α, and SODs. Noteworthy, our IHC results show an especially high concentration of SOD2 in activated glia surrounding amyloid plaques, whilst SOD1 is scarcely present in these cells, consistent with our previous light and electron microscopic observations [66]. The critical role of SODs in AD progression is well documented and emphasised by reports on deletion versus overexpression of the respective genes [38, 39, 67].

5. Conclusions

In this work we report age-related molecular changes occurring in the neocortex of the Tg2576 mouse model of AD, with a focus on oxidative stress. Our results confirm and extend previous observations from others’ and our own groups, supporting the view that the chosen model is eminently suited to reveal the earliest signs of the disease, even at a preclinical stage [9, 10, 22, 29, 30]. This goal is crucial to dissect the molecular mechanisms underlying Aβ pathology onset, with the ultimate goal of developing novel therapeutic strategies to prevent, or at least to slow, disease progression.

Our present data, reporting defective antioxidant defences and cytoplasmic nucleic acid oxidative damage and altered redox status sensors in Tg neurons, starting from 3 months of age, support the hypothesis that oxidative stress and mitochondrial dysfunction are early, interrelated pathogenetic factors [35, 36, 68]. Since the primary culprit of the disease, at least in our model, remains Aβ overproduction, it will be of utmost interest to study even earlier stages, considering that congenital expression of mutated APP may lead to accumulation of toxic peptides during pre-, peri-, or early postnatal brain development. On the other hand, the opportunity this AD model offers to study pathogenetic mechanisms over a relatively long-time scale [69] allowed us to follow the gradual, though dramatic, changes of oxidative stress-related molecules in the neocortex. Overall, our data demonstrate that the ability to trigger a compensatory response is conserved until 9 months of age, while at later stages all antioxidant defences appear irreversibly lost. These results are in general agreement with the vast literature on this topic, even though time sequence of oxidative stress may differ, depending on the mouse model, gender, and brain region considered [70].

Interestingly, our present and previous [10, 22] data point not only to mitochondria, but also to peroxisomes, as organelles involved in the response to the redox unbalance characterizing the earliest phases of Aβ pathology. In fact, both organelles, which are functionally interconnected, reportedly generate, respond to, and are affected by oxidative stress mediators, in physiopathological conditions [71–73]. On the other hand, at more advanced stages of disease, peroxisomes, possibly enhancing their functions in astroglia, may play a protective role, by supporting neurons with fatty acid-derived energy fuel. This phenomenon, witnessed by the significant increase in PMP70 at 9 months, coincides with the activation of astrocytes, known to be endowed with an abundant peroxisomal population. Therefore, our study suggests that therapeutic designing against AD should consider an additional target, that is, peroxisomes. As a matter of fact, peroxisome proliferators, particularly PPARα natural and synthetic agonists, have been demonstrated to control glucose, lipid, and lactate homeostasis and to exert neuroprotective actions [19, 74–76]. However, the complex heterogeneity of pathological changes occurring in AD requires that any therapeutic effort have a multitargeted approach [77]. Thus, pharmacological treatments should be directed not only to protect from oxidative damage, but also to support mitochondria and peroxisomes in their energy metabolism related functions. Also, attention should be paid to both neurons and astrocytes, for their cooperation in these pathways. It remains that the primary goal to pursue is to catch the disease at its first, subtle, and hardly recognised signs [78].

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Authors’ Contribution

Sara Porcellotti, Francesca Fanelli, and Anna Fracassi equally contributed to the work.

Acknowledgments

The authors wish to thank Professor Alfred Völkl (University of Heidelberg, Germany) for generously providing them with the anti-acyl CoA oxidase, Professor Ralph Erdmann (Ruhr University Bochum, Bochum, Germany) for anti-Pex14p, Professor Paul Van Veldhoven (Catholic University of Leuven, Belgium) for anti-thiolase, and Professor Koji Uchida (Nagoya University, Aichi, Japan), for anti-acrolein. The authors are indebted to Francesca Greco, for technical and imaging assistance. The technical staff of UOC Pathological Anatomy of San Filippo Neri Hospital is also gratefully acknowledged for skillful assistance. This work was partially supported by grants to Sandra Moreno from University Roma Tre (“Internationalization and Research Training Project” and “CAL”) and by FP-6 Integrated European Project LSHG-CT-512018.

References

H. W. Querfurth and F. M. LaFerla, “Alzheimer's disease,” The New England Journal of Medicine, vol. 362, no. 4, pp. 329–344, 2010.
View at: Publisher Site | Google Scholar
D. M. Walsh and D. J. Selkoe, “Aβ oligomers—a decade of discovery,” Journal of Neurochemistry, vol. 101, no. 5, pp. 1172–1184, 2007.
View at: Publisher Site | Google Scholar
K. Bettens, K. Sleegers, and C. van Broeckhoven, “Genetic insights in Alzheimer's disease,” The Lancet Neurology, vol. 12, no. 1, pp. 92–104, 2013.
View at: Publisher Site | Google Scholar
G. A. Elder, M. A. Gama Sosa, and R. de Gasperi, “Transgenic mouse models of Alzheimer's disease,” Mount Sinai Journal of Medicine, vol. 77, no. 1, pp. 69–81, 2010.
View at: Publisher Site | Google Scholar
K. Hsiao, P. Chapman, S. Nilsen et al., “Correlative memory deficits, Aβ elevation, and amyloid plaques in transgenic mice,” Science, vol. 274, no. 5284, pp. 99–102, 1996.
View at: Publisher Site | Google Scholar
J. S. Jacobsen, C.-C. Wu, J. M. Redwine et al., “Early-onset behavioral and synaptic deficits in a mouse model of Alzheimer's disease,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 13, pp. 5161–5166, 2006.
View at: Publisher Site | Google Scholar
M. C. Irizarry, M. McNamara, K. Fedorchak, K. Hsiao, and B. T. Hyman, “APPSW transgenic mice develop age-related Aβ deposits and neuropil abnormalities, but no neuronal loss in CA1,” Journal of Neuropathology & Experimental Neurology, vol. 56, no. 9, pp. 965–973, 1997.
View at: Publisher Site | Google Scholar
M. A. Westerman, D. Cooper-Blacketer, A. Mariash et al., “The relationship between Aβ and memory in the Tg2576 mouse model of Alzheimer's disease,” The Journal of Neuroscience, vol. 22, no. 5, pp. 1858–1867, 2002.
View at: Google Scholar
M. D'Amelio, V. Cavallucci, S. Middei et al., “Caspase-3 triggers early synaptic dysfunction in a mouse model of Alzheimer's disease,” Nature Neuroscience, vol. 14, no. 1, pp. 69–79, 2011.
View at: Publisher Site | Google Scholar
F. Fanelli, S. Sepe, M. D'Amelio et al., “Age-dependent roles of peroxisomes in the hippocampus of a transgenic mouse model of Alzheimer's disease,” Molecular Neurodegeneration, vol. 8, article 8, 2013.
View at: Publisher Site | Google Scholar
R. M. J. Deacon, L. L. Cholerton, K. Talbot et al., “Age-dependent and -independent behavioral deficits in Tg2576 mice,” Behavioural Brain Research, vol. 189, no. 1, pp. 126–138, 2008.
View at: Publisher Site | Google Scholar
Y. Zhao and B. Zhao, “Oxidative stress and the pathogenesis of Alzheimer's disease,” Oxidative Medicine and Cellular Longevity, vol. 2013, Article ID 316523, 10 pages, 2013.
View at: Publisher Site | Google Scholar
P. H. Reddy, “Misfolded proteins, mitochondrial dysfunction, and neurodegenerative diseases,” Biochimica et Biophysica Acta, vol. 1842, no. 8, p. 1167, 2014.
View at: Publisher Site | Google Scholar
D. Trompier, A. Vejux, A. Zarrouk et al., “Brain peroxisomes,” Biochimie, vol. 98, no. 1, pp. 102–110, 2014.
View at: Publisher Site | Google Scholar
J. Clark and D. K. Simon, “Transcribe to survive: transcriptional control of antioxidant defense programs for neuroprotection in Parkinson's disease,” Antioxidants & Redox Signaling, vol. 11, no. 3, pp. 509–528, 2009.
View at: Publisher Site | Google Scholar
J. N. Feige, L. Gelman, L. Michalik, B. Desvergne, and W. Wahli, “From molecular action to physiological outputs: peroxisome proliferator-activated receptors are nuclear receptors at the crossroads of key cellular functions,” Progress in Lipid Research, vol. 45, no. 2, pp. 120–159, 2006.
View at: Publisher Site | Google Scholar
T. Wenz, “Mitochondria and PGC-1α in aging and age-associated diseases,” Journal of Aging Research, vol. 2011, Article ID 810619, 12 pages, 2011.
View at: Publisher Site | Google Scholar
M. T. Heneka, E. Reyes-Irisarri, M. Hüll, and M. P. Kummer, “Impact and therapeutic potential of PPARs in Alzheimer's disease,” Current Neuropharmacology, vol. 9, no. 4, pp. 643–650, 2011.
View at: Publisher Site | Google Scholar
M. Fidaleo, F. Fanelli, M. Cerù, and S. Moreno, “Neuroprotective properties of peroxisome proliferator-activated receptor Alpha (PPARα) and its lipid ligands,” Current Medicinal Chemistry, vol. 21, no. 24, pp. 2803–2821, 2014.
View at: Publisher Site | Google Scholar
L. Katsouri, K. Blondrath, and M. Sastre, “Peroxisome proliferator-activated receptor-γ cofactors in neurodegeneration,” International Union of Biochemistry and Molecular Biology Life, vol. 64, no. 12, pp. 958–964, 2012.
View at: Publisher Site | Google Scholar
A. Bagattin, L. Hugendubler, and E. Mueller, “Transcriptional coactivator PGC-1α promotes peroxisomal remodeling and biogenesis,” Proceedings of the National Academy of Sciences of the United States of America, vol. 107, no. 47, pp. 20376–20381, 2010.
View at: Publisher Site | Google Scholar
A. Cimini, S. Moreno, M. D'Amelio et al., “Early biochemical and morphological modifications in the brain of a transgenic mouse model of Alzheimer's disease: a role for peroxisomes,” Journal of Alzheimer's Disease, vol. 18, no. 4, pp. 935–952, 2009.
View at: Publisher Site | Google Scholar
M. M. Bradford, “A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein dye binding,” Analytical Biochemistry, vol. 72, no. 1-2, pp. 248–254, 1976.
View at: Publisher Site | Google Scholar
M. Hartlage-Rübsamen, M. Morawski, A. Waniek et al., “Glutaminyl cyclase contributes to the formation of focal and diffuse pyroglutamate (pGlu)-Aβ deposits in hippocampus via distinct cellular mechanisms,” Acta Neuropathologica, vol. 121, no. 6, pp. 705–719, 2011.
View at: Publisher Site | Google Scholar
S. Moreno, S. Farioli-vecchioli, and M. P. Cerù, “Immunolocalization of peroxisome proliferator-activated receptors and retinoid X receptors in the adult rat CNS,” Neuroscience, vol. 123, no. 1, pp. 131–145, 2004.
View at: Publisher Site | Google Scholar
M. Morita and T. Imanaka, “Peroxisomal ABC transporters: structure, function and role in disease,” Biochimica et Biophysica Acta, vol. 1822, no. 9, pp. 1387–1396, 2012.
View at: Publisher Site | Google Scholar
C. W. T. van Roermund, L. Ijlst, T. Wagemans, R. J. A. Wanders, and H. R. Waterham, “A role for the human peroxisomal half-transporter ABCD3 in the oxidation of dicarboxylic acids,” Biochimica et Biophysica Acta—Molecular and Cell Biology of Lipids, vol. 1841, no. 4, pp. 563–568, 2014.
View at: Publisher Site | Google Scholar
E. Benedetti, B. D'Angelo, L. Cristiano et al., “Involvement of peroxisome proliferator-activated receptor β/δ (PPAR β/δ) in BDNF signaling during aging and in Alzheimer disease: possible role of 4-hydroxynonenal (4-HNE),” Cell Cycle, vol. 13, no. 8, pp. 1335–1344, 2014.
View at: Publisher Site | Google Scholar
F. Tamagnini, C. Burattini, T. Casoli, M. Balietti, P. Fattoretti, and G. Aicardi, “Early impairment of long-term depression in the perirhinal cortex of a mouse model of Alzheimer's disease,” Rejuvenation Research, vol. 15, no. 2, pp. 231–234, 2012.
View at: Publisher Site | Google Scholar
A. M. Duffy, J. Morales-Corraliza, K. M. Bermudez-Hernandez et al., “Entorhinal cortical defects in Tg2576 mice are present as early as 2–4 months of age,” Neurobiology of Aging, vol. 36, no. 1, pp. 134–148, 2015.
View at: Publisher Site | Google Scholar
J. Lalande, H. Halley, S. Balayssac et al., “1H NMR metabolomic signatures in five brain regions of the aβPPswe Tg2576 mouse model of Alzheimer's disease at four ages,” Journal of Alzheimer's Disease, vol. 39, no. 1, pp. 121–143, 2014.
View at: Publisher Site | Google Scholar
M. J. Callahan, W. J. Lipinski, F. Bian, R. A. Durham, A. Pack, and L. C. Walker, “Augmented senile plaque load in aged female β-amyloid precursor protein-transgenic mice,” The American Journal of Pathology, vol. 158, no. 3, pp. 1173–1177, 2001.
View at: Publisher Site | Google Scholar
J. St-Pierre, S. Drori, M. Uldry et al., “Suppression of reactive oxygen species and neurodegeneration by the PGC-1 transcriptional coactivators,” Cell, vol. 127, no. 2, pp. 397–408, 2006.
View at: Publisher Site | Google Scholar
A. Nunomura, G. Perry, G. Aliev et al., “Oxidative damage is the earliest event in Alzheimer disease,” Journal of Neuropathology & Experimental Neurology, vol. 60, no. 8, pp. 759–767, 2001.
View at: Google Scholar
A. M. Swomley, S. Förster, J. T. Keeney et al., “Abeta, oxidative stress in Alzheimer disease: evidence based on proteomics studies,” Biochimica et Biophysica Acta—Molecular Basis of Disease, vol. 1842, no. 8, pp. 1248–1257, 2014.
View at: Publisher Site | Google Scholar
X. Wang, W. Wang, L. Li, G. Perry, H. G. Lee, and X. Zhu, “Oxidative stress and mitochondrial dysfunction in Alzheimer's disease,” Biochimica et Biophysica Acta—Molecular Basis of Disease, vol. 1842, no. 8, pp. 1240–1247, 2014.
View at: Publisher Site | Google Scholar
M. Y. Aksenov, H. M. Tucker, P. Nair et al., “The expression of key oxidative stress-handling genes in different brain regions in Alzheimer's disease,” Journal of Molecular Neuroscience, vol. 11, no. 2, pp. 151–164, 1998.
View at: Publisher Site | Google Scholar
C. A. Massaad, R. G. Pautler, and E. Klann, “Mitochondrial superoxide: a key player in Alzheimer's disease,” Aging, vol. 1, no. 9, pp. 758–761, 2009.
View at: Google Scholar
M. Dumont, E. Wille, C. Stack, N. Y. Calingasan, M. F. Beal, and M. T. Lin, “Reduction of oxidative stress, amyloid deposition, and memory deficit by manganese superoxide dismutase overexpression in a transgenic mouse model of Alzheimer's disease,” The FASEB Journal, vol. 23, no. 8, pp. 2459–2466, 2009.
View at: Publisher Site | Google Scholar
J. Hroudová, N. Singh, and Z. Fišar, “Mitochondrial dysfunctions in neurodegenerative diseases: relevance to alzheimer's disease,” BioMed Research International, vol. 2014, Article ID 175062, 9 pages, 2014.
View at: Publisher Site | Google Scholar
J. M. Flynn and S. Melovn, “SOD2 in mitochondrial dysfunction and neurodegeneration,” Free Radical Biology & Medicine, vol. 62, pp. 4–12, 2013.
View at: Publisher Site | Google Scholar
M. E. Poynter and R. A. Daynes, “Peroxisome proliferator-activated receptor α activation modulates cellular redox status, represses nuclear factor-κB signaling, and reduces inflammatory cytokine production in aging,” The Journal of Biological Chemistry, vol. 273, no. 49, pp. 32833–32841, 1998.
View at: Publisher Site | Google Scholar
C. Scuderi, G. Esposito, A. Blasio et al., “Palmitoylethanolamide counteracts reactive astrogliosis induced by β-amyloid peptide,” Journal of Cellular and Molecular Medicine, vol. 15, no. 12, pp. 2664–2674, 2011.
View at: Publisher Site | Google Scholar
C. Scuderi, M. Valenza, C. Stecca, G. Esposito, M. R. Carratù, and L. Steardo, “Palmitoylethanolamide exerts neuroprotective effects in mixed neuroglial cultures and organotypic hippocampal slices via peroxisome proliferator-activated receptor-α,” Journal of Neuroinflammation, vol. 9, article 49, 2012.
View at: Publisher Site | Google Scholar
G. D'Agostino, R. Russo, C. Avagliano, C. Cristiano, R. Meli, and A. Calignano, “Palmitoylethanolamide protects against the amyloid-β25-35-induced learning and memory impairment in mice, an experimental model of alzheimer disease,” Neuropsychopharmacology, vol. 37, no. 7, pp. 1784–1792, 2012.
View at: Publisher Site | Google Scholar
M. Cuadrado-Tejedor, J. F. Cabodevilla, M. Zamarbide, T. Gómez-Isla, R. Franco, and A. Pérez-Mediavilla, “Age-related mitochondrial alterations without neuronal loss in the hippocampus of a transgenic model of Alzheimer's disease,” Current Alzheimer Research, vol. 10, no. 4, pp. 390–405, 2013.
View at: Publisher Site | Google Scholar
G. Leipnitz, A. U. Amaral, C. G. Fernandes et al., “Pristanic acid promotes oxidative stress in brain cortex of young rats: a possible pathophysiological mechanism for brain damage in peroxisomal disorders,” Brain Research, vol. 1382, pp. 259–265, 2011.
View at: Publisher Site | Google Scholar
E. N. B. Busanello, A. U. Amaral, A. M. Tonin et al., “Experimental evidence that pristanic acid disrupts mitochondrial homeostasis in brain of young rats,” The Journal of Neuroscience Research, vol. 90, no. 3, pp. 597–605, 2012.
View at: Publisher Site | Google Scholar
G. Lizard, O. Rouaud, J. Demarquoy, M. Cherkaoui-Malki, and L. Iuliano, “Potential roles of peroxisomes in Alzheimer's disease and in dementia of the Alzheimer's type,” Journal of Alzheimer's Disease, vol. 29, no. 2, pp. 241–254, 2012.
View at: Publisher Site | Google Scholar
M. Fransen, M. Nordgren, B. Wang, O. Apanasets, and P. P. van Veldhoven, “Aging, age-related diseases and peroxisomes,” Subcellular Biochemistry, vol. 69, pp. 45–65, 2013.
View at: Google Scholar
D. Praticò, K. Uryu, S. Leight, J. Q. Trojanoswki, and V. M.-Y. Lee, “Increased lipid peroxidation precedes amyloid plaque formation in an animal model of alzheimer amyloidosis,” The Journal of Neuroscience, vol. 21, no. 12, pp. 4183–4187, 2001.
View at: Google Scholar
M. Singh, D. T. Nam, M. Arseneault, and C. Ramassamy, “Role of by-products of lipid oxidation in Alzheimer's disease brain: a focus on acrolein,” Journal of Alzheimer's Disease, vol. 21, no. 3, pp. 741–756, 2010.
View at: Publisher Site | Google Scholar
S. J. Baloyannis, “Mitochondrial alterations in Alzheimer's disease,” Journal of Alzheimer's Disease, vol. 9, no. 2, pp. 119–126, 2006.
View at: Google Scholar
T. Kawarabayashi, L. H. Younkin, T. C. Saido, M. Shoji, K. H. Ashe, and S. G. Younkin, “Age-dependent changes in brain, CSF, and plasma amyloid β protein in the Tg2576 transgenic mouse model of Alzheimer's disease,” Journal of Neuroscience, vol. 21, no. 2, pp. 372–381, 2001.
View at: Google Scholar
S. Desagher, J. Glowinski, and J. Premont, “Astrocytes protect neurons from hydrogen peroxide toxicity,” The Journal of Neuroscience, vol. 16, no. 8, pp. 2553–2562, 1996.
View at: Google Scholar
S. Moreno, E. Mugnaini, and M. P. Cerù, “Immunocytochemical localization of catalase in the central nervous system of the rat,” Journal of Histochemistry & Cytochemistry, vol. 43, no. 12, pp. 1253–1267, 1995.
View at: Publisher Site | Google Scholar
B. Ahlemeyer, I. Neubert, W. J. Kovacs, and E. Baumgart-Vogt, “Differential expression of peroxisomal matrix and membrane proteins during postnatal development of mouse brain,” Journal of Comparative Neurology, vol. 505, no. 1, pp. 1–17, 2007.
View at: Publisher Site | Google Scholar
C. Masters, “Gluconeogenesis and the peroxisome,” Molecular and Cellular Biochemistry, vol. 166, no. 1-2, pp. 159–168, 1997.
View at: Publisher Site | Google Scholar
G. A. Brooks, “Cell-cell and intracellular lactate shuttles,” The Journal of Physiology, vol. 587, no. 23, pp. 5591–5600, 2009.
View at: Publisher Site | Google Scholar
F. Ding, J. Yao, J. R. Rettberg, S. Chen, and R. D. Brinton, “Early decline in glucose transport and metabolism precedes shift to ketogenic system in female aging and Alzheimer's mouse brain: Implication for bioenergetic intervention,” PLoS ONE, vol. 8, no. 11, Article ID e79977, 2013.
View at: Publisher Site | Google Scholar
J. Apelt, M. Bigl, P. Wunderlich, and R. Schliebs, “Aging-related increase in oxidative stress correlates with developmental pattern of beta-secretase activity and beta-amyloid plaque formation in transgenic Tg2576 mice with Alzheimer-like pathology,” International Journal of Developmental Neuroscience, vol. 22, no. 7, pp. 475–484, 2004.
View at: Publisher Site | Google Scholar
M. Pekny, U. Wilhelmsson, and M. Pekna, “The dual role of astrocyte activation and reactive gliosis,” Neuroscience Letters, vol. 565, pp. 30–38, 2014.
View at: Publisher Site | Google Scholar
P. Agostinho, R. A. Cunha, and C. Oliveira, “Neuroinflammation, oxidative stress and the pathogenesis of Alzheimer's disease,” Current Pharmaceutical Design, vol. 16, no. 25, pp. 2766–2778, 2010.
View at: Publisher Site | Google Scholar
Y. Yao, C. Chinnici, H. Tang, J. Q. Trojanowski, V. M. Y. Lee, and D. Praticò, “Brain inflammation and oxidative stress in a transgenic mouse model of Alzheimer-like brain amyloidosis,” Journal of Neuroinflammation, vol. 1, no. 1, article 21, 2004.
View at: Publisher Site | Google Scholar
H. Johnston, H. Boutin, and S. M. Allan, “Assessing the contribution of inflammation in models of Alzheimer's disease,” Biochemical Society Transactions, vol. 39, no. 4, pp. 886–890, 2011.
View at: Publisher Site | Google Scholar
S. Moreno, R. Nardacci, and M. P. Cerù, “Regional and ultrastructural immunolocalization of copper-zinc superoxide dismutase in rat central nervous system,” Journal of Histochemistry & Cytochemistry, vol. 45, no. 12, pp. 1611–1622, 1997.
View at: Publisher Site | Google Scholar
K. Murakami, N. Murata, Y. Noda et al., “SOD1 (copper/zinc superoxide dismutase) deficiency drives amyloid β protein oligomerization and memory loss in mouse model of Alzheimer disease,” The Journal of Biological Chemistry, vol. 286, no. 52, pp. 44557–44568, 2011.
View at: Publisher Site | Google Scholar
Z. Chen and C. Zhong, “Oxidative stress in Alzheimer's disease,” Neuroscience Bulletin, vol. 30, no. 2, pp. 271–281, 2014.
View at: Publisher Site | Google Scholar
J. E. Lee and P. L. Han, “An update of animal models of Alzheimer disease with a reevaluation of plaque depositions,” Experimental Neurobiology, vol. 22, no. 2, pp. 84–95, 2013.
View at: Publisher Site | Google Scholar
A. Belkacemi and C. Ramassamy, “Time sequence of oxidative stress in the brain from transgenic mouse models of Alzheimer's disease related to the amyloid-β cascade,” Free Radical Biology & Medicine, vol. 52, no. 3, pp. 593–600, 2012.
View at: Publisher Site | Google Scholar
H. K. Delille, R. Alves, and M. Schrader, “Biogenesis of peroxisomes and mitochondria: linked by division,” Histochemistry and Cell Biology, vol. 131, no. 4, pp. 441–446, 2009.
View at: Publisher Site | Google Scholar
S. Thoms, S. Grønborg, and J. Gärtner, “Organelle interplay in peroxisomal disorders,” Trends in Molecular Medicine, vol. 15, no. 7, pp. 293–302, 2009.
View at: Publisher Site | Google Scholar
B. Wang, P. P. Van Veldhoven, C. Brees et al., “Mitochondria are targets for peroxisome-derived oxidative stress in cultured mammalian cells,” Free Radical Biology & Medicine, vol. 65, pp. 882–894, 2013.
View at: Publisher Site | Google Scholar
I. Paterniti, M. Cordaro, M. Campolo et al., “Neuroprotection by association of palmitoylethanolamide with luteolin in experimental Alzheimer's disease models: the control of neuroinflammation,” CNS & Neurological Disorders—Drug Targets, vol. 13, no. 9, pp. 1530–1541, 2014.
View at: Publisher Site | Google Scholar
C. Scuderi, C. Stecca, M. Valenza et al., “Palmitoylethanolamide controls reactive gliosis and exerts neuroprotective functions in a rat model of Alzheimer’s disease,” Cell Death & Disease, vol. 5, article e1419, 2014.
View at: Publisher Site | Google Scholar
E. Aso and I. Ferrer, “Cannabinoids for treatment of alzheimer's disease: moving toward the clinic,” Frontiers in Pharmacology, vol. 5, article 37, Article ID Article 37, 2014.
View at: Publisher Site | Google Scholar
N. Sato and R. Morishita, “Roles of vascular and metabolic components in cognitive dysfunction of Alzheimer disease: short- and long-term modification by non-genetic risk factors,” Frontiers in Aging Neuroscience, vol. 5, 2013.
View at: Publisher Site | Google Scholar
D. J. Selkoe, “Preventing alzheimer's disease,” Science, vol. 337, no. 6101, pp. 1488–1492, 2012.
View at: Publisher Site | Google Scholar

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Copyright © 2015 Sara Porcellotti et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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