Background
Accumulating evidence suggests that neuroinflammation is a common pathological feature of tauopathy, characterized with intracellular accumulation of tau proteins in neurodegenerative disorders such as Alzheimer’s disease (AD) [
1]. Microglia, the resident macrophages in the brain, are the primary immune cells responsible for the detection of invading pathogens and neuronal injuries in the central nervous system (CNS) [
2]. Activated microglia are observed in the postmortem brain tissues of various human tauopathies including Alzheimer’s disease [
3]. Microglial cells can be activated not only by injury and infection [
4] but also by stimulators including amyloid beta (Aβ) [
5] and serum amyloid A (SAA) [
6]. Activated microglial cells in turn exhibit dramatic morphological changes, proliferate, migrate, and produce a variety of pro- and anti-inflammatory mediators [
4,
7] such as interleukin-1 (IL-1), IL-6, and IL-18, which accelerate tauopathy including the formation of neurofibrillary tangles (NFTs) [
8‐
11]. Although these findings suggest a possible link between neuroinflammation and tauopathy, there is little evidence for direct regulation of activated microglia in the pathological accumulation of the microtubule-associated protein tau.
Human SAA is a family of proteins consisting of SAA1, SAA2, and SAA4 [
12]. Among these proteins, SAA1 and SAA2 are the major acute-phase proteins primarily synthesized by hepatocytes during acute-phase response [
13]. However, extrahepatic production of SAA has been implicated as being more relevant to the pathogenesis of chronic inflammatory diseases including AD [
13]. In mice, SAA is encoded by a family of three inducible genes, Saa1, Saa2, and Saa3, plus a constitutively expressed Saa4. The major site of their synthesis is the liver; however, Saa3 is also expressed in extrahepatic tissues in response to lipopolysaccharide (LPS) stimulation [
14]. SAA has cytokine-like properties that modulate several cellular responses. SAA induces monocytes and neutrophils migration and stimulates the production of cytokines, chemokines, and matrix metalloproteinases (MMPs) [
15‐
20]. Although the inducible SAA proteins are barely detectable in normal brains, SAA has been found in the brains of patients with AD [
13,
21]. Moreover, SAA has been found to colocalize with Aβ deposits in AD brains [
22], and the induction of a systemic acute-phase response in SAA transgenic mice enhances amyloid deposition [
23]. Despite these findings, a correlation between SAA and tauopathy has not been established.
In this study, we found that the expression of the mouse SAA protein, Saa3, in the mouse brain was markedly increased in a LPS injection model of systemic inflammation. We evaluated the effects of SAA on tau phosphorylation in Saa3 gene knockout (Saa3
−/−) mice with systemic LPS injection and in mice receiving intracerebral injection of SAA. The results have shown that the SAA proteins significantly attenuate tau hyperphosphorylation in these mouse models. Moreover, SAA has been found to regulate the activation of microglia in these mouse models. Finally, we have observed that IL-10 released from SAA-stimulated microglia attenuates tau hyperphosphorylation in neurons. Based on these findings, we postulate that SAA plays a role in tauopathy in part through the regulation of microglia activation.
Methods
Reagents
Primary antibodies used in this study are listed in Additional file
1: Table S1. The BCA protein assay kit and 4,6-diamidino-2-phenylindole (DAPI) were obtained from Beyotime Institute of Biotechnology (Nantong, Jiangsu, China). Mouse and rabbit control IgGs were purchased from Santa Cruz Biotechnology (Dallas, TX). IRDye®800CW secondary antibodies were from LI-COR (Lincoln, NE). Dulbecco’s modified Eagle’s medium (DMEM), neurobasal-A, and B-27® supplements were purchased from Life Technologies (Carlsbad, CA). Other chemicals were obtained from Sigma Chemical Company (St. Louis, MO).
Animals
The
Saa3
−/− (
Saa3 knockout) mice in C57BL/6 genetic background were obtained from the Knockout Mouse Project (KOMP) Repository (Davis, CA). Age- and sex-matched littermates were used in the experiments. The C57BL/6 mice were purchased from SLACCAS Laboratory Animal Co., Ltd (Shanghai, China). The generation of the Saa3 transgenic mice is described in Additional file
2. All mice were housed (four to five animals per cage) with a 12/12 h light/dark cycle, with ad libitum access to food and water. The housing, breeding, and animal experiments were in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals, with procedures approved by the Biological Research Ethics Committee of Shanghai Jiao Tong University.
LPS administration
Lipopolysaccharide (LPS, from Salmonella enterica serotype Abortus equi, Sigma-Aldrich, Cat. No. L5886, Lot 032M4067) at a low concentration (5 mg/kg body weight) or a high concentration (15 mg/kg body weight) was intraperitoneally injected into 3-month-old C57BL/6 mice consisting of Saa3
−/− and their respective wild-type (WT) littermates (n = 4 per group; half males and half females). The mice received either LPS or an equal volume of normal saline. After 24 h, all mice were sacrificed by decapitation and their brains removed immediately. The hippocampi and cerebral cortices of the left hemisphere of the mouse brain were dissected, flash frozen in dry ice, and stored at −80 °C for biochemical analyses later. The right hemispheres of the mouse brains were fixed with 4 % paraformaldehyde in 0.1 M phosphate-buffered saline (PBS), followed by cryoprotection in 30 % sucrose. Coronal sections of 30-μm thickness were cut using a freezing sliding microtome. The sections were stored in glycol anti-freeze solution (ethylene glycol, glycerol, and 0.1 M PBS in 3:3:4 ratio) at −20 °C until immunohistochemical staining.
Stereotaxic intracranial injection of SAA
Three-month-old C57BL/6 mice were randomly divided into control (saline) and SAA (recombinant human apo-SAA; Pepro Tech, Rocky Hill, NJ) (
n = 4 in each group; half males and half females). Mice were anesthetized by intraperitoneal injection of 50 mg/kg pentobarbital sodium (Sigma) and then restrained onto a stereotaxic apparatus (RWD Life Science, Shenzhen, China). For stereotaxic intracranial injection of SAA, an earlier method was used [
24]. After surgically exposed, the duramater and drilled holes in the skull, SAA (20 μg/8 μl) dissolved in saline was bilaterally injected into the left and right hippocampi (two sites, 4 μl per site), using a 10-μl Hamilton syringe with a 26-gauge needle. The injection rate was 0.5 μl/min, and the needle was kept in each site for an additional 3 min before a gentle withdrawal. The bregma coordinates were determined as follows: anterior, −2.0 mm; lateral, ±1.3 mm; vertical, −2.2 mm. As controls, the mice stereotaxically received equal volume of normal saline. Postoperatively, all mice were placed on heating pads (37 °C) until recovered from surgery. After 48 h, the injected mice were sacrificed by decapitation and the brain samples were prepared as with the LPS-treated mice described above.
For brain injection of SAA with IL-10 neutralizing antibody (BD Pharmingen, San Diego, CA), SAA (10 μg per site, two sites) with IL-10 neutralizing antibody (4 μg per site, two sites) were stereotaxically injected into the left and right hippocampi of the 3-month-old C57BL/6 mice (n = 4 in each group; half males and half females). As controls, the mice received an equal volume of SAA dissolved in saline (20 μg/8 μl) or normal saline alone (8 μl). After 48 h, the injected mice were sacrificed by decapitation and the brain samples were prepared as with the LPS-treated mice described above.
Total RNA extraction and real-time PCR
Total RNA was extracted from the cortex and hippocampus of the mouse brain and primary cultures of neurons, astrocytes, and microglial cells using TRIzol reagent (Invitrogen). One microgram of the RNA was used for reverse transcription using the Reverse Transcription System A3500 kit (Promega, Madison, WI). The complementary DNA (cDNA) was subsequently subjected to Real-Time PCR to quantify the transcripts of TNF-α, IL-6, IL-10, Saa1, and Saa2, and Saa3 using SYBR® Green Real-time PCR Master Mix (TOYOBO, Osaka, Japan). The following primers were used: TNF-α (5′-TTC TCA TTC CTG CTT GTG G-3′; 5′-ACT TGG TGG TTT GCT ACG-3′), IL-6 (5′-CTT CTT GGG ACT GAT G-3′; 5′-CTG GCT TTG TCT TTC T-3′), IL-10 (5′-AGG GTT ACT TGG GTT GC-3′; 5′-TGA GGG TCT TCA GCT TC-3′), Saa1 (5′-TTG TTC ACG AGG CTT TC-3′; 5′-TTT GTC AGG CAG TCC AG-3′), Saa2 (5′-TGA TGC TGC CCA AAG G-3′; 5′-GCC AGG AGG TCT GTA GTA A-3′), and Saa3 (5′-CCT TCC ATT GCC ATC A-3′; 5′-GGG TCT TTG CCA CTC C-3′). The primers for the mouse housekeeping gene glyceraldehyde-3-phosphate dehydrogenase (GAPDH) were 5′-CCT TCC GTG TTC CTA CC-3′ and 5′-CAA CCT GGT CCT CAG TGT A-3′. PCR was performed according to the following conditions: 94 °C for 3 min, 40 cycles of denaturation at 94 °C for 30 s, annealing at 56 °C for 45 s, and extension at 72 °C for 30 s, followed by a final extension at 72 °C for 10 min. The quantitative fold changes in messenger RNA (mRNA) in each sample were normalized to GAPDH expression and calculated using the 2exp(−ΔΔCt) method.
Western blot analysis
Mouse brain tissues and cultured neuronal cells were homogenized in lysis buffer containing 50 mM Tris-HCl (pH 7.4), 8.5 % sucrose, 1.0 mM EGTA, 1.0 mM EDTA, 1.0 % sodium dodecylsulfate, 10 mM β-mercaptoethanol, protease, and phosphatase inhibitor cocktails (Sigma-Aldrich). Protein concentrations were determined using a BCA Protein Assay Kit (Beyotime Biotechnology, Nantong, China) and then heated in 5×SDS-PAGE loading buffer (Beyotime Biotechnology) at 99 °C for 7 min. Tissue and neuronal cell homogenates were separated on 10 or 12 % SDS-PAGE and transferred onto nitrocellulose membranes (Whatman Protran, Dassel, Germany). Blots were blocked with 5 % non-fat milk for 1 h at room temperature and incubated overnight at 4 °C with primary antibodies including Tau5 (1:2000); the anti-phospho-tau antibodies pS199 (1:2000), pS205 (1:2000), pS396 (1:2000), pS404 (1:2000), anti-Saa3(1:500), and anti-β-actin (1:10000), followed by the respective IRDye®800CW secondary antibodies (LI-COR Biosciences, Lincoln, NE). The membranes were scanned using the 800-nm channel of an Odyssey® CLX Infrared Imaging System. The immunoreactive bands were quantified using the NIH Image J software.
Immunofluorescence staining
Sections of mouse brain were washed with 0.05 M Tris-buffered saline (TBS) (containing 0.05 M Tris buffer and 9 g/L NaCl, pH 7.4) for 15 min and then permeabilized with 0.1 % Triton X-100 in TBS for 15 min and blocked with 5 % normal goat serum (NGS) for 30 min at room temperature. The sections were incubated overnight at 4 °C with anti-Iba1 (1:500) in TBS with 5 % NGS. After washing with TBS for 15 min, the sections were incubated with Alex Fluor®568 donkey anti-rabbit antibody (1:500, Invitrogen) at room temperature for 1 h. Again, after three washes in TBS, the sections were stained for nuclei with 5 μg/ml of DAPI for 10 min at room temperature and mounted on glass slides. To identify the expression of Saa3 in neuron, microglia, or astrocyte, the brain sections were first stained with anti-MAP-2 (1:200), anti-CD11b (1:200), or anti-glial fibrillary acidic protein (GFAP)-Cy3TM (1:500) antibody overnight and incubated in Alex Fluor®633 donkey anti-mouse or Alex Fluor®555donkey anti-rat IgG (1:500; Invitrogen) for 1 h. The sections were rinsed in TBS, stained with anti-Saa3 antibody (1:200) overnight at 4 °C, and incubated with an Alex Fluor®488 donkey anti-rabbit antibody (1:500; Invitrogen) for 1 h. Sections were counterstained with DAPI for 10 min, and then fluorescent confocal images were captured using a laser-scanning confocal fluorescence microscope (TCS SP8, Leica Microsystems, Wetzlar, Germany).
Images for the quantification of fluorescence intensity of Saa3, CD11b and GFAP were acquired at ×400 magnification. The relative immunofluorescence intensity of Saa3, CD11b, and GFAP was quantified using the ImageProPlus Software (Media Cybernetics, Silver Spring, MD). The results were expressed as mean ± SEM based on a minimum of three sections per animal and three 8-bit RGB digital images at the CA1 per animal (n = 4 mice per group).
To exclude obscure influence of Saa3 on microglial proliferation, the number of Iba1-positive cells was taken into consideration. Integrated optical density of red fluorescence (Iba1 positive area capture) was normalized against the integrated optical density of blue fluorescence (the DAPI positive area captured), using the Image ProPlus 6.0 software and expressed as mean ± SEM per group (three sections per animal, with images acquired at ×200 magnification; three 8-bit RGB digital images at the dentate gyrus (DG) and CA3 region per animal; n = 4).
Primary neuronal cultures
Neuronal cultures were prepared in cortices from newborn (postnatal day 0) WT mouse pups as described before [
25]. In brief, cerebral cortices were removed from the brains of mice, the meanings and microvessels were removed, and tissues were minced with a sterile razor blade. Tissues were digested with 0.025 % trypsin (Sigma) and 0.01 % DNase I (Sigma) at 37 °C for 10 min. The cell suspension was filtered through a 200-mesh sieve, and cells were plated on poly-
d-lysine (Sigma)-coated 24-well plates at a density of 5 × 10
5 cells per well. Two hours later, the DMEM medium was replaced with neurobasal medium containing 2 % B-27® supplements for 2 days. Culture medium were changed to neurobasal with 10 % fetal bovine serum (FBS) and 3 μg/ml cytosine-β-D-arabinofuranoside (Ara-C, Sigma) in the following 3 days and then again switched back to neurobasal medium containing 2 % B-27® supplements. Experiments were performed on days 7–8 after initiation of the culture.
Primary microglial and astrocyte cultures
Microglial and astrocyte cultures were prepared from newborn (postnatal day 0) WT mouse pups as described before [
6,
25,
26]. Specifically, separated cells were cultured in poly-D-lysine coated 75 cm
2 flasks with DMEM medium (containing 10 % FBS, 100 U/ml penicillin, and 100 g/ml streptomycin sulfate). The medium was replenished on day 1 and day 3. On day 7, microglia cells in the culture flasks were shaken off at 260 rpm for 2.5 h, and the remaining astrocytes were maintained in DMEM with 10 % FBS. Experiments were performed after two passages of the cells.
SAA and LPS treatment in vitro
Primary neuronal cells, astrocyte cells, and microglial cells were stimulated with LPS at indicated concentrations or with PBS for 24 h. Total RNA was extracted for real-time PCR to detect cell-specific expression of Saa3. For the analysis of the effect of SAA on neuronal tau phosphorylation, primary neuronal cells were treated with the recombinant human SAA (PeproTech, Rocky Hill, NJ; 0.5 μΜ for 3, 6 and 12 h), and the neuronal lysates were prepared for Western blot analysis as mentioned above.
Preparation of conditioned media from microglia and astrocytes
The microglia cells and astrocyte were plated at a density of 1 × 106 cells per well onto a 12-well plate for experiments involving the collection of conditioned media. The cells were treated with 0.5 μΜ SAA or PBS (control) for 6 h. The medium was removed and replaced with fresh DMEM. The cells were incubated for another 12 h, and the conditioned medium (CM) was collected. Half of the medium in the primary neurons was replaced with equal volume of CM from SAA-stimulated or PBS (control) cell culture. After 3, 6, and 12 h of incubation, neuronal lysate was prepared and blotted for Western analysis. To determine the effect of IL-10, an IL-10-neutralizing antibody (25 μg/ml; BD Pharmingen, San Diego, CA) was added to CM 30 min before application to primary cultures of neurons. After 12 h of incubation, neuronal lysate was prepared and Western blot analysis was conducted.
ELISA
The IL-10 in the microglial conditioned medium was measured using enzyme-linked immunosorbent assay (ELISA) kit (eBioscience, San Diego, CA), according to the instructions of the vender. Briefly, the conditioned medium and mouse IL-10 standard samples were incubated in the IL-10 ELISA plates at 4 °C overnight. After washed plates three times with PBST (PBS + 0.5 % Tween-20) and blocked with 3 % BSA in PBS for 1 h at 37 °C, biotin-conjugate anti-mouse IL-10 antibody was incubated in the wells at 37 °C for 90 min. The plate was emptied and washed three times with PBST. Substrate solution was pipetted into each well after drying and incubated in 37 °C for 10 min. The enzymatic reaction was stopped by adding stop solution per well. The concentration of IL-10 was determined by measuring absorbance at 450 and 630 nm. All the experiments were done in three separate experiments.
Statistical analysis
Data are presented as mean ± SEM from at least three experiments. One-way ANOVA followed by Newman-Keuls test or student’s t test was performed using the statistic software GraphPad Prism 5 (San Diego, CA). p values less than 0.05 was considered statistically significant.
Discussion
The present study brings two new findings. One is a suppressive function of brain SAA in tau hyperphosphorylation, and the other is the involvement of microglia in this function. The majority of the published studies show that intracellular neurofibrillary tangles (NFTs) often accompany microglia activation [
29], suggesting a possible link between activated microglia and tau phosphorylation. However, except studies showing that altered microglia activation play a role in modulating tau hyperphosphorylation within neurons via the CX3CL1-CX3CR1 interaction [
30,
31], there has been no direct evidence for an effect of microglia activation in tau hyperphosphorylation. Our previous study found that SAA induces changes in the morphology, survival, and cytokine production in murine microglia, indicating that it plays a role in the activation of microglia [
6]. The present study demonstrated for the first time that SAA is involved in the regulation of microglia activation and in modulating tau phosphorylation using different mouse models. Our experimental data confirmed that IL-10 released from the SAA-stimulated microglia could affect tau hyperphosphorylation in cultured primary neurons. Collectively, these results provide new evidence for an indirect mechanism by which SAA modulates AD-related pathologies.
In the present study, we evaluated the effect of SAA on tau hyperphosphorylation using the mouse model of systemic LPS administration. LPS has been widely utilized in mouse models to induce neuroinflammation via either systemic administration or direct injection into the brain [
30,
32‐
35]. Notably, several recent studies showed that the acute effect of LPS can induce tau hyperphosphorylation in the mouse brain and worsen the tau pathology in Tau-Tg mice or 3xTg mice [
30,
32,
36‐
39]. Consistent with these published studies, we found that a single dose of LPS given peripherally is sufficient to induce neuroinflammation and tau hyperphosphorylation. Furthermore, using
Saa3
−/− mice, our studies demonstrate that the LPS-induced changes in tau phosphorylation are altered in
Saa3-deficient mice. These findings provide first evidence for a potential role of the SAA proteins in LPS-induced tau hyperphosphorylation.
The present study also provides the first documentation of local expression and distribution of SAA isoforms in the mouse brain. We found that Saa3 is the predominant SAA isoform induced by systemic LPS administration in the mouse brain. As a result of this finding,
Saa3 was chosen for further analysis using a gene knockout approach. Because Saa3 is less well characterized for its regulatory functions compared to the acute-phase SAA of human origin (SAA1 and SAA2), we have included in our study a human SAA protein in intracerebral injection and in the stimulation of cultured brain cells. Both experiments have given results that complement each other and together support a regulatory role of SAA in tau phosphorylation. We have also found that a significant amount of the induced Saa3 protein is in neurons and, to a much lesser extent, astrocytes in the DG region of hippocampus and in the cortex. However, SAA expression is negligible in microglia under the same experimental conditions. This finding is unexpected as previously published studies have shown that macrophages, which share many properties with microglia, are a source of SAA proteins [
40]. The discrepancy may result from the efficiency of Saa3 translation in different types of cells and from the difference in the in vivo (brain sections) and in vitro (cultured cells) experimental conditions.
Despite the lack of SAA production by microglia, these cells can nevertheless respond to SAA stimulation with the release of factors that regulate tau hyperphosphorylation in neurons. In comparison, neurons fail to respond to SAA directly in assays for tau phosphorylation, suggesting that the neuron-derived SAA acts through a paracrine mechanism that involves a mediator. IL-10 is an anti-inflammatory cytokine known for its inhibition of Aβ- and LPS-induced pro-inflammatory cytokines and chemokines in the brain [
41]. Two studies have shown that down-regulation of tau phosphorylation is accompanied by up-regulation of IL-10 [
42,
43], suggesting a possible link between IL-10 and tau phosphorylation. In the present study, we demonstrated that IL-10 released by SAA-stimulated microglia attenuates tau phosphorylation in neurons, and neutralizing IL-10 could reverse the decrease of tau phosphorylation induced by intracerebral SAA injection in mice. These results provide additional evidence for an effect of IL-10 on tau phosphorylation. Therefore, IL-10 serves to mediate the function of SAA, which acts indirectly. A previous example of the indirect action is reported by Harrison et al., who document that CX3CL1 is produced by neurons in the brain and signals through CX3CR1, which is expressed in microglia [
44,
45]. More interestingly, Kevin Nash et al. found that overexpression CX3CL1 in the rTg4510 mouse model directly suppresses tauopathies [
46]. Together, these results provide evidence for the indirect regulatory mechanism of microglial cells in modulating tau phosphorylation and indicate that glial cell regulation may be a potential therapeutic strategy for tauopathies.
Previous study from our laboratory demonstrated that SAA administration could induce significant activation of primary microglial cells in culture [
6]. Consistent with this finding, in the present study, stereotaxic hippocampal injection of SAA induced microglia activation in the mouse brain. These findings suggest that the regulatory function of SAA may depend on the activation states of microglia. Both the present study and our previous study [
6] show that SAA can induce the release of pro-inflammatory cytokines including IL-1β, IL-6, and TNF-α, as well as the anti-inflammatory cytokine IL-10. The pro-inflammatory cytokines and anti-inflammatory cytokines released from SAA-stimulated microglia may contribute to the homeostatic function of SAA in the brain. It is through the action of the anti-inflammatory cytokine IL-10 that SAA exerts its regulatory effect on tau phosphorylation. Future studies will be required to illuminate whether and how other cytokines released by activated microglia also contribute to the regulation of tau phosphorylation and how SAA-mediated activation of microglia plays a role in this process.
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
JL, DW, and SQL performed the in vivo and in vitro studies including cell isolation and culture, measurement of tau phosphorylation, and generation of confocal microscopic images. JL and YY processed and analyzed data. YY and RDY designed the study and wrote the manuscript. All authors have read and agreed with the contents of the manuscript.