- Open Access
Interleukin-10 deficiency exacerbates inflammation-induced tau pathology
Journal of Neuroinflammation volume 18, Article number: 161 (2021)
The presence of hyperphosphorylated microtubule-associated protein tau is strongly correlated with cognitive decline and neuroinflammation in Alzheimer’s disease and related tauopathies. However, the role of inflammation and anti-inflammatory interventions in tauopathies is unclear. Our goal was to determine if removing anti-inflammatory interleukin-10 (IL-10) during an acute inflammatory challenge has any effect on neuronal tau pathology.
We induce systemic inflammation in Il10-deficient (Il10−/−) versus Il10+/+ (Non-Tg) control mice using a single intraperitoneal (i.p.) injection of lipopolysaccharide (LPS) to examine microglial activation and abnormal hyperphosphorylation of endogenous mouse tau protein. Tau phosphorylation was quantified by Western blotting and immunohistochemistry. Microglial morphology was quantified by skeleton analysis. Cytokine expression was determined by multiplex electro chemiluminescent immunoassay (MECI) from Meso Scale Discovery (MSD).
Our findings show that genetic deletion of Il10 promotes enhanced neuroinflammation and tau phosphorylation. First, LPS-induced tau hyperphosphorylation was significantly increased in Il10−/− mice compared to controls. Second, LPS-treated Il10−/− mice showed signs of neurodegeneration. Third, LPS-treated Il10−/− mice showed robust IL-6 upregulation and direct treatment of primary neurons with IL-6 resulted in tau hyperphosphorylation on Ser396/Ser404 site.
These data support that loss of IL-10 activates microglia, enhances IL-6, and leads to hyperphosphorylation of tau on AD-relevant epitopes in response to acute systemic inflammation.
Alzheimer’s disease (AD) is one of the tauopathies and the most common neurodegenerative disease involving the abnormal phosphorylation and accumulation of the microtubule-associated protein tau (MAPT or tau). Tau is a neuron-enriched protein known to bind and stabilize microtubules under homeostatic conditions and has non-microtubule-binding functions [1, 2]. However, in tauopathies, tau acquires abnormal toxic forms via various post-translational modifications that lead to loss of tau’s function or gain of toxic function [2,3,4]. The presence of hyperphosphorylated tau has been shown to strongly correlate with cognitive decline [5,6,7] and neuroinflammation [8, 9]. Increasing evidence suggests neuroinflammation is a major component of tauopathies including AD [10, 11]. Additionally, previous studies suggest that activated (pro-inflammatory) microglia are sufficient to induce hyperphosphorylation of tau both in vivo and in vitro . Furthermore, in vivo animal models suggest that inflammation precedes and contributes to tau pathology . Therefore, understanding the role of anti-inflammatory molecules is important in thwarting excessive neuroinflammation that contributes to tau pathology relevant to AD and related tauopathies.
Interleukin-10 (IL-10) is a well-establishedanti-inflammatory cytokine with an important role in preventing unrestrained inflammatory responses from activated immune cells [13, 14]. The central nervous system (CNS) resident cells, microglia and astrocytes, are both major producers of IL-10, in vitro . However, a recent single cell transcriptome analysis of IL-10 production in microglia raises questions about whether microglia produce IL-10 after endotoxin challenge, in vivo . IL-10 plays a role in downregulating inflammatory responses in a variety of cell types  including microglia in the brain . Furthermore, a known single nucleotide polymorphism in the promoter region of Il10 is associated with abnormal hippocampus-dependent memory function  and increased risk for AD in human subjects [20,21,22]. Therefore, the potential of IL-10 in reducing brain inflammation and subsequent tau pathology is understudied and important to determine in the context of AD. Interestingly, a compelling study by Chackrabarty et al. has suggested that adeno-associated viral vector-mediated overexpression of IL-10 in amyloid-precursor protein (APP) mouse model of AD exacerbated amyloid pathology and cognitive impairment due to stunted phagocytic ability of microglia [23, 24]. However, it is still unclear whether or not IL-10 plays any regulatory role in tau pathology. Based on this, we hypothesized that IL-10 plays a role in regulating the pro-inflammatorypathway that contributes to tau phosphorylation within the brain.
In the current study, we sought to determine if IL-10 suppresses inflammation leading to tau pathology in a model of acute systemic inflammation induced by lipopolysaccharide (LPS). We have shown that LPS-induced microglial activation promotes hyperphosphorylation of tau in non-transgenic mice through toll-like receptor 4 (TLR4) signaling. In our previous study, 1 mg/kg b.w. of LPS did not induce significant increases in AT8 or AT180 tau phosphorylation compared to vehicle-treated controls, and even 10 mg/kg b.w. of LPS had only a moderate increase in pTau in the wild-type mice . This suggests a homeostatic control mechanism potentially regulated by an anti-inflammatory cytokine, such as IL-10, may exist. However, mice lacking microglial fractalkine receptor (CX3CR1) showed robust microglial activation and increased tau phosphorylation after systemic LPS treatment, supporting the importance of microglial involvement in driving tau pathology. Notably, the microglia-induced neuroinflammation and tau pathology was mediated via interleukin-1β, (IL-1β) and activation of p38 mitogen-activated protein kinase (p38 MAPK) pathway . Here, to determine the contributions from IL-10 in regulated microglia-mediated tau pathology, we compared inflammatory responses in the brains of Il10-deficient (Il10−/−) versus Il10+/+ (Non-Tg) control mice using a moderate dose of LPS to induce systemic inflammation. We examined microglial activation and phosphorylation of tau in the hippocampi after 24 h of LPS treatment. We predicted that lack of IL-10 would exacerbate an ongoing inflammatory response to promote hyperphosphorylation of tau.
B6.129P2-Il10tm1Cgn/J (Il10−/−)  and C57BL/6J mice (Non-Tg) were both in the C57BL/6J genetic background obtained from the Jackson Laboratory (JAX stock #002251 and #000664). All experimental protocols involving animals were performed in accordance with the US National Institutes of Health guidelines on animal care and were approved (16-200428-BHSC; 15-200352-HSC) by the Institutional Animal Care and Use Committees of the University of New Mexico.
Vehicle (Veh, Hank’s balanced saline solution, HBSS) or lipopolysaccharide (LPS, Sigma #L2880) from Escherichia coli 055:B5 was administered (3 mg/kg body weight, b.w.; intraperitoneally, i.p.; single dose) to 5–6-month-old non-transgenic or Il10−/− mice on C57BL/6J background. After 24 h, the mice were sacrificed, and brain tissue was collected as described below. LPS concentration is based on previous papers showing the efficacy of this dose to induce tau phosphorylation in the hippocampi of wild-type mice .
Brain tissue collection and preparation
Mice were anesthetized, transcardially perfused with 0.125 M phosphate buffer (PB) and brains were removed. Left hemispheres were fixed in 4% paraformaldehyde in PB (4% PFA/PB), incubated in cryoprotection solution for 24 h, sliced into 30μm thick sagittal brain sections, and stored at -20°C in cryostorage solution until use in TUNEL and immunohistochemical analysis. Right hemispheres were micro-dissected into cortex, hippocampus, and the rest of the brain, wet weights were recorded, and the tissues were snap frozen in liquid nitrogen. The cortices and hippocampi were used in biochemical protein analysis.
Multiplex electrochemiluminescent immunoassay
Cortical tissue sections were homogenized in a buffered sucrose solution containing protease and phosphatase inhibitors and processed for protein analysis as previously described [28,29,30]. Tissue homogenates were spun at 4200×g at 4 °C for 10 min. Protein concentrations of cortical lysates were determined by Bradford protein assay (Biorad). A total of 200 μg of protein/sample in duplicate was used to determine cytokine levels using multiplex electrochemiluminescent immunoassay (MECI). The V-PLEX Plus Proinflammatory Panel 1 (mouse) electrochemiluminescent immunoassay platform (MesoScale Discovery #K15048G, MesoScale Diagnostics LLC) was used to detect multiple cytokines, including IL-10, IL-12p70, IL-1β, TNF-α, IL-6, and the chemokine, CXCL1. Plates were read on a Quickplex SQ 120 Imager.
Hippocampal tissues were homogenized in Tissue-Protein Extraction Reagent, TPER (ThermoScientific, #78510) with protease and phosphatase inhibitor cocktails. The tissue homogenates were sonicated and spun at 13,700×g at 4 °C for 30 min. The soluble fraction was diluted with NuPage LDS Sample Buffer and Sample Reducing Agent, run on 4–12% Bis-Tris Novex NuPage gels (Invitrogen) for 1 h. Proteins were transferred from the gel to PVDF membranes overnight. Membranes were washed and blocked in 5% milk/PBS blocking buffer and incubated overnight in primary antibodies. Membranes were washed and incubated for 1 h in corresponding HRP-conjugated secondary antibodies (Jackson ImmunoResearch Laboratories, Inc. #115-035-146 and #111-035-144). Membranes were incubated with ECL reagent (ThermoScientific) and exposed to X-ray film. Immunoreactive bands on the developed film were scanned and quantified with AlphaEaseFCTM Software (Alpha Innotech Corporation).
For in vivo experiments: Western blots were probed for phosphorylated tau antibodies: PHF-1 (1:10,000, a generous gift from Dr. Peter Davies); AT180 (1:5000), AT8 (1:10,000), and total tau Tau5 (1:10,000) (Thermo Scientific); and activated phospho-p38 MAPK (1:500) and total p38 MAPK (1:1000) (Cell Signaling); and loading control, glyceraldehyde-3-phosphate dehydrogenase (GAPDH) (1:20,000; Millipore).
For in vitro experiments: Western blots were probed for phosphorylated tau antibodies: PHF-1 (1:5,000); AT8 (1:5,000); Tau5 (1:5,000); GAPDH (1:10,000), activated phospho-p38 MAPK (1:500) and total p38 MAPK (1:1000) (Cell Signaling); and activated phospho-STAT3 and STAT3 (1:2000, Cell Signaling) to verify intracellular neuronal signaling downstream of IL-6.
Free-floating sections were processed via standard immunohistochemical methods. Briefly, a sodium citrate solution was used for antigen retrieval, endogenous peroxidases were blocked with 3% H2O2 in PBST, and 5% normal goat serum in Triton/PBS was used as blocking buffer. Primary antibody incubation was overnight at 4°C. Incubation with corresponding Biotinylated IgG secondary antibodies (Jackson ImmunoResearch Laboratories, Inc. #115-065-003 and #111-065-144) was for 1 h. Sections were then incubated with Avidin:Biotinylated enzyme complex reagent and developed using SIGMAFASTTM3,3′-Diaminobenzidine (DAB) tablets (Sigma, D4293) without metal enhancer to reveal immunoreactive signals. IHC brain sections were probed for phosphorylated tau, AT180 (1:250, Thermo Scientific), and microglia, ionized calcium-binding adapter molecule 1 (Iba1) (1:500, Wako).
For terminal deoxynucleotidyl transferase dUTP nick end labeling (TUNEL) assay, staining was performed using the protocol supplied with a Roche in situ cell death detection kit (Roche Applied Science # 11684809910). Sections were co-stained with NeuN (1:250) (Cell Signaling) to visualize neurons. The percent area of TUNEL+ staining of pyknotic neuronal bodies was imaged and quantified using fluorescent microscopy and threshold analysis in ImageJ.
Quantifying microglia morphology
ImageJ Skeleton Analysis was based on procedures previously described . Briefly, fixed brain sections were prepared by immunohistochemistry and stained with Iba1, as described above. Brightfield photograph images (40×) of Iba1-stained sagittal brain sections were processed into binary skeletonized images using ImageJ with the following steps. First, images were run through a bandpass filter and converted to grayscale, automatic brightness/contrast was applied, followed by the Unsharp Mask filter and Despeckle tools for removing noise. Auto-threshold was applied to create a black and white image contrast of the microglia. An additional despeckle step followed by “binary-close” and “noise-remove outliers” functions (as described in the published protocol) results in removing noise and closing gaps in the microglial processes. Finally, we skeletonize the image using the Skeletonize and Analyze Skeleton functions in ImageJ.
Primary neuron culture and treatments
Primary neuron cultures were prepared following an established protocol . Briefly, early postnatal (P0-P1) mouse (C57BL/6j) hippocampi and cortices were isolated, rinsed, trypsinized, dissociated and plated on prepared poly-L-lysine coated coverslips. Within two days after plating, cytosine arabinoside (araC; 1-b-d-arabinofuranosylcytosin) is added to inhibit proliferating non-neuronal cells resulting in a predominantly neuronal cell population. Cultures were grown for 16 days in vitro (DIV) at 37°C in humidified 5% CO2 incubator prior to any treatment. DIV 16 cultures were treated with 25 ng/mL recombinant mouse IL-6 (Biolegend) and collected in LDS/RA solution 12 h after treatment. Collected cell lysates in LDS/RA were sonicated and boiled before use in western immunoblot assay.
Adult neuron isolation and treatments
Dissociation of adult mouse brains was performed using the “Adult Brain Dissociation Kit for mouse and rat” (Miltenyi Biotec, 130-107-677) and “Neuron Isolation Kit for mouse” (Miltenyi Biotec, 130-115-389) following the user manual, in combination with the gentleMACS Dissociator (Miltenyi Biotec). Mice were anesthetized and the brains removed then cut into 8 sagittal slices. Brain slices were homogenized using the gentle MACS Dissociator in C Tubes (Miltenyi Biotec, 130-093-237) with the recommended volume of enzyme mixes. Tissue was processed with no modification to the protocol in the kit. Isolated neurons from the adult mouse brains were cultured for one week changing half the media (MACS Neuro Medium containing 2% MACS Neuro Brew-21,1% penicillin/streptomycin, and 0.5 mM l-glutamine) every other day. One week after neuronal isolation, neurons were treated with 25 ng/mL recombinant mouse IL-6 (Biolegend) and collected in LDS/RA solution 12 h after treatment. Collected cell lysates in LDS/RA were sonicated and boiled before use in western immunoblot assay.
Unless otherwise indicated, comparisons between the two groups were done via unpaired t test. Comparisons between multiple treatment groups were done via one-way or two-way analysis of variance (ANOVA) with Sidak’s multiple comparison post hoc test. All statistical analyses were performed using GraphPad Prism® (Version 8).
Genetic deletion of Il10 promotes tau hyperphosphorylation after peripheral LPS administration
Abnormal hyperphosphorylation of tau is regarded as an early hallmark of AD [33, 34]. Well-characterizedAD-relevant phosphorylated tau epitopes at Ser202/Thr205, Thr231, and Ser396/Ser404 detected by AT8, AT180, and PHF-1 antibodies, respectively, can serve as markers for tau pathology [35,36,37]. Protein analysis via Western blot of hippocampal lysates from Il10−/− and Non-Tg mice was performed to determine the levels of tau phosphorylation at AT8, AT180, and PHF-1 epitopes 24 h following one dose of intraperitoneal LPS injection (Fig. 1A–D). No significant differences were found in the basal levels of phosphorylated tau (pTau) or total tau between Il10−/− and Non-Tg mice treated with Veh. However, 24 h following LPS-injection, both the Il10−/− and Non-TgLPS-treated groups had increased AT8+ and AT180+ pTau. Importantly, the Il10−/− LPS mice had significant increases in AT8+, AT180+, and PHF-1+ pTau compared to the Non-Tg LPS mice (Fig. 1B–D). Notably, total tau levels were significantly reduced in Il10−/− mice after LPS administration (Fig. 1E) compared to Il10−/− Veh mice and Non-TgLPS-treated mice. These data suggest that deficiency of IL-10 exacerbates hyperphosphorylation of tau in the hippocampus within 24 h of LPS administration.
To verify the spatial distribution of phosphorylated tau in different sub-regions within the dentate gyrus of the mouse brains, immunohistochemistry (IHC) of sagittal brain sections was performed. Quantification of AT180+ area, 24 h post-LPS treatment, confirmed significantly enhanced pTau in the dentate gyrus of Il10−/− mice compared to Non-Tg mice (Fig. 2A, B). The morphology of the AT180+ area resembled neuronal cell bodies rather than astrocytes or oligodendrocytes, which can also abnormally harbor pTau [38,39,40]. These results confirm significantly increased phosphorylated tau epitopes in hippocampal neurons of Il10−/− mice.
LPS-treated Il10 −/− mice show signs of neurodegeneration
We speculated that a loss of total tau mentioned above is most likely due to neuronal death since tau is highly enriched in neurons . To evaluate the possibility of neuronal cell death within the hippocampi of the LPS-injected mice, neuronal cell death was examined using TUNEL assay. There was notable detection of TUNEL positive cells (green) colocalized with NeuN+ neurons (red) that appeared to have yellowish nuclei (arrows) in the CA3 hippocampal regions of Il10−/− LPS mice compared to the Veh and Non-Tg LPS groups (Fig. 2C). Quantification confirmed the increased number of TUNEL+ cells in the neuronal layer of Il10−/− LPS mice compared to the Veh and Non-Tg LPS groups (Fig. 2D). These data corroborate neuronal cell death in Il10−/− LPS mice, which is consistent with the significant reduction in neuron-enriched tau protein.
Il10deficiency enhances LPS-induced p38 MAPK activation
Activated p38 MAPK is a member of the MAPK family and key signal transduction protein involved in CNS inflammation  and implicated in tau phosphorylation [12, 42,43,44,45,46]. To determine if activated p38 MAPK was elevated in the Il10−/− mice, we examined levels of phosphorylated p38 MAPK (phospho-Thr180/Tyr182) in the hippocampal lysates (Fig. 3). Basal levels of phospho-p38 were no different in Il10−/− mice vs Non-Tg mice and LPS administration did not significantly elevate levels of active p38 MAPK in LPS-injectedNon-Tg mice (Fig. 3A, B). However, robust and statistically significant phospho-p38 MAPK activation was observed in LPS-injectedIl10−/− mice compared to the LPS-injectedNon-Tg control group (Fig. 3A, B). No statistically significant differences in the total p38 ratio over GAPDH were observed in either genotypes or treatment groups when assessed by two-way ANOVA (Fig. 3C). These data suggest IL-10 deficiency alters active forms of p38 MAPK and, in the context of an inflammatory response, correlates with enhanced tau phosphorylation and neurodegeneration.
Il10-deficient microglia display activated morphology with LPS treatment
Next, we wanted to assess the microglial phenotype in Il10−/− mice after LPS administration to reassert the role of reactive microglia in driving pTau. Brain sections were stained with Iba1 to visualize microglial morphology (Fig. 4A) and a skeleton analysis was performed to quantify the branching (data not shown) and junctions of microglial processes in the hippocampus (Fig. 4B). We observed that Il10−/− Veh mouse brains already had a slightly elevated, though not statistically significant, Iba1+ area compared to Non-Tg Veh controls. Interestingly, the Il10−/− Veh microglia in the CA1 region had slightly increased branching (data not shown) and significantly increased the number of junctions compared to the other groups (Fig. 4D). After LPS administration, we observed that the Iba1+ area increased in both groups, suggesting a more activated phenotype than vehicle-treated respective control (Fig. 4C). Notably, there was no significant enhancement of Iba1 expression attributed to IL-10 deficiency after LPS administration. However, analysis of the skeletonized branching of the microglia revealed that Il10−/− microglia had significantly reduced branching (data not shown) and decreased the number of junctions compared to Non-Tg microglia post-LPS (Fig. 4D). This suggests a more amoeboid, highly activated phenotype resembling pro-inflammatory microglia in the LPS-treatedIl10−/− mice brains compared to LPS-treatedNon-Tg controls.
Il10 deficiency significantly enhanced inflammatory cytokines
Cytokine levels in cortical tissue lysates from Il10−/− and Non-Tg mouse brains were examined to confirm the pro-inflammatory phenotype. First, basal levels of IL-10 were below the level of detection in both groups prior to LPS. Basal levels of IL-12, IL-1β, and TNFα were low and not significantly different in Il10−/− mice vs Non-Tg controls. Slightly elevated levels of IL-10 were still detectable in a number of LPS-treatedNon-Tg mice 24 h after the LPS challenge whereas IL-10 remained below background levels of detection in LPS-treatedIl10−/− mice (Fig. 5A). Additionally, the Non-Tg group had elevated levels of IL-1β, TNFα, and IL-6 after LPS administration (Fig. 5C–E). In comparison, Il10−/− mice had significantly enhanced levels of IL-12, TNFα, and IL-6 relative to Non-Tg controls (Fig. 5B, D, E). Out of all four pro-inflammatory cytokines studied, a thousand-fold elevated increase in IL-6 levels that remained elevated at 24 h post-LPS injection in LPS-treatedIl10−/− mice was very striking (Fig. 5E). Surprisingly, IL-1β was not found to be significantly elevated in the LPS Il10−/− mice compared to LPS-treatedNon-Tg controls at this 24 h timepoint (Fig. 5B).
Direct stimulation of primary neurons with IL-6 induces tau hyperphosphorylation
Since IL-6 was expressed by more than a thousand-fold increase in LPS-treatedIl10−/− mice compared to LPS-treatedNon-Tg controls, we evaluated the potential role of IL-6 on tau phosphorylation in murine primary neurons. First, we treated mouse primary neuronal cultures derived from P0 C67BL/6j pups with recombinant IL-6 and performed Western blot analysis for phospho-tau in the cell lysates. We verified that activated STAT3 (phospho-tyr705) levels were significantly elevated in IL-6-treated neurons (Fig. 6A–D) indicating expected intracellular response downstream of IL-6 signaling. Next, we observed a modest increase in the AT8/Tau5 and AT8/GAPDH ratios in IL-6-treated neurons compared to vehicle-treated controls. Importantly, PHF-1/Tau5 and PHF-1/GAPDH ratios were significantly higher in IL-6 stimulated neurons relative to Veh controls (Fig. 6A–D). Interestingly, similar to the trends we observed with the in vivo results, there was a modest reduction in total tau (Tau5/GAPDH ratio) and an increase in p-p38/total-p38 MAPK ratio in the IL6-treated neurons (Fig. 6A–D). Furthermore, stimulation of neurons derived from adult IL-10 knockout mice with IL-6 showed significantly elevated levels of PHF-1/Tau5 ratio compared to adult non-transgenic neurons treated with IL-6 (Fig. 6E–F). This suggests that IL-6 is sufficient to promote increased tau phosphorylation within neurons and it is enhanced in neurons deficient in IL-10.
In this study, we demonstrate that deficiency of IL-10 was sufficient to increase tau hyperphosphorylation after only 24 h of a moderate dose of LPS treatment. We observed tau phosphorylation was enhanced in Il10−/− mice treated with LPS. We detected reduced total tau and increased neuronal cell death in hippocampi of LPS-treatedIl10−/− mice. We confirmed that an important tau kinase, p38 MAPK, was activated in hippocampal tissue of Il10−/− mice after LPS administration and significantly enhanced in the LPS-treatedIl10−/− mice compared to LPS-treatedNon-Tg controls. Il10−/− microglia had morphological features of activated amoeboid cells, along with upregulation of pro-inflammatory cytokines, IL-12, TNFα, and IL-6, after LPS treatment. Particularly, IL-6 was substantially increased in the LPS-treatedIl10−/− mice and we demonstrated that direct stimulation with IL-6 is sufficient to induce tau phosphorylation in a primary mouse neuronal culture. These data substantiate a role for IL-10 in regulating the inflammatory response to an immune challenge through TLR4 signaling that involves p38 MAPK, microglial activation, and excessive pro-inflammatory cytokine expression, which results in hyperphosphorylation of tau.
IL-10 dysregulation is highly relevant to AD in a number of ways. First, there are single nucleotide polymorphisms (SNPs) in the Il10 promoter associated with increased risk of AD [22, 47]. For example, the ATA haplotype (−1082A/−819 T/−592A) of the IL-10 gene promoter region is associated with susceptibility to AD [20, 48]. Particularly, an “A” allele at position 1082 has been associated with low production of IL-10  and is implicated in promoting mild cognitive impairment (MCI) to AD [19, 47]. In line with the association of low IL-10 production with AD, patients with faster rates of decline in their mini-mental state exams (MMSE) were shown to have significantly lower production of IL-10 upon ex vivo peripheral blood mononuclear cell (PBMC) stimulation, suggesting that IL-10 expression could be protective in the slow declining population . Our study corroborates the concept of IL-10 dysfunction leading to an increased pathology related to AD.
Second, IL-10 regulates microglial phenotype and immune processes, which are implicated in AD. According to a recent genome-wide association study (GWAS) by the International Genomics of Alzheimer’s Project, some of the most influential risk factors for AD compared to controls were in genotypes associated with microglia and the immune system [51, 52]. Furthermore, animal studies have shown that reactive microglia are sufficient to drive tau pathology [12, 53] but the role of pro- and anti-inflammatory mediators on microglial phenotype and function is still being understood. Dysregulated IL-10 expression has been shown to alter microglial phenotype through both overexpression and deficiency [54, 55] but there are still conflicting data on how IL-10 influences microglial function. For example, in the context of amyloid plaque clearance, it has been shown that IL-10 dampens β-amyloid clearance and IL-10 deficiency permits β-amyloid phagocytosis by microglia [24, 56]. On the other hand, a recent in vitro study suggests that IL-10 promotes phagocytosis dependent on the triggering receptor expressed on myeloid cells 2 (TREM2) in microglia . IL-10 deficiency, in our LPS model, promoted a highly activated, pro-inflammatory microglial phenotype. Interestingly, the microglia in our Veh-treatedIl10−/− mice, which are deficient in IL-10 throughout their life, seemingly had an intermediate stage of activation (increased Iba1 and hypertrophic processes) in the hippocampus CA1, but not the CA3, region. Thus, discerning the effects of dysregulated IL-10 on AD may require an understanding of intermediate activation states of microglia, the microglial microenvironment, and the dosage as well as the timing of IL-10.
Finally, dysregulation of cytokines, including IL-10, is implicated in AD. For example, inflammasome signaling molecules are increased in AD brains  and colocalize with microglia around plaques . Furthermore, patients with advanced rates of progression from MCI to dementia in AD have elevated levels of pro-inflammatory cytokines in the CSF . Although IL-10 is also found to be upregulated in the CSF of AD patients , it is concomitant with elevation in pro-inflammatory cytokine levels. This is in line with the role of IL-10 in negative feedback inhibition in response to inflammatory stimuli [17, 61]. On the same note, we saw that the absence of IL-10 lead several cytokines, including TNFα and IL-6, to run rampant after the LPS challenge. IL-10 signaling through the IL-10 receptor in microglia involves activation of the JAK/STAT/SOCS pathway  resulting in IL-10 induced genes. This includes dual-specificity phosphatases (DUSP), which downregulates p38 MAPK activation in myeloid cells [63, 64]. In line with this, we saw that the absence of IL-10 lead to increased p38 MAPK activation. IL-10 has been shown to regulate the expression of a number of pro-inflammatory cytokines in microglial cultures and brain tissue [15, 65, 66]. This includes IL-1β, which can peak at 5 h in the brain after peripheral LPS administration in rodents  but has complex endotoxin-dependentIL-1β maturation kinetics depending on extracellular ATP release . Interestingly, we observed that IL-1β cytokine expression did not remain significantly elevated in Il10−/− mice compared to Non-Tg mice at 24 h after LPS administration. This may suggest another compensatory mechanism limited the ongoing expression of IL-1β within 24 h in our model. However, we do not know the relative expression levels of IL-1β at earlier timepoints and cannot rule out a role for IL-1β in promoting tau hyperphosphorylation in this model. Potentially, there are multiple routes leading to AD-relevant tau phosphorylation if left unregulated. In our study, TNFα and IL-6, were particularly elevated by LPS in the absence of IL-10. Interestingly, IL-6 remained significantly elevated in the Il10−/− mice, which alludes to clinical correlations between genotypes associated with low IL-10 and high IL-6 production as a risk factor for AD [21, 68, 69]. Therefore, we explored the potential for IL-6 to promote tau phosphorylation in neurons by directly stimulating neuron-enriched primary cultures with recombinant IL-6.IL-6 stimulation was sufficient to induce tau phosphorylation in primary hippocampal neurons consistent with a previous study that showed IL-6 stimulation increased neuronal pTau . Interestingly, the study by Quintanilla et al., showed that treatment of primary hippocampal rat neurons with 5 ng/mL IL-6 significantly increased phosphorylated tau (AT8/Tau5 ratio) and lowered unphosphorylated tau (Tau1/Tau5 ratio) after a 48-h incubation. In our study, treatment of primary hippocampal mouse neurons with 25 ng/mL of IL-6 for 12 h significantly increased tau phosphorylation on the Ser396/Ser404 (PHF-1) epitope and total tau (Tau5/GAPDH) was significantly decreased. These data support a role for dysregulated cytokines, including IL-10 and IL-6, in promoting AD-relevant tau phosphorylation. It is important to note that our results do not show elevated cytokine levels in IL-10 knockout mice with LPS is cell-autonomous to microglia. As such, at this stage, it is still correlational and require single cell RNA sequencing and profiling of microglia based on their cytokine expression phenotype. Performing such studies is beyond the scope of the present study and our future studies will determine if disease-associated microglia (DAMs), interferon-responsive microglia (IRMs), and other types of microglia relevant to AD/tauopathies are specifically altered in IL-10 knockout mice brains with LPS challenge.
The role that inflammation plays and whether it contributes to AD has increasingly become an important area of research due to increased evidence that microglial activation and abnormal expression of cytokines are associated with AD. Understanding inflammatory pathways that promote tauopathy is necessary to find novel targets for AD. Here, we provide evidence that IL-10 deficiency enhances a pro-inflammatory environment in the brain after a peripheral immune challenge leading to hyperphosphorylation of tau on AD-relevant epitopes. Our model involves inducing inflammation through TLR4 signaling using LPS as the stimulus. Immune activation through TLR4 is relevant in AD as amyloid beta (Aβ), is known to trigger TLR4 signaling to secrete inflammatory factors [71, 72]. TLR4 can also be triggered by danger-associated molecular patterns (DAMPs) due to neuronal injury and other tissue damage . Therefore, this model pertains to TLR4 signaling promoting tauopathy and is not strictly pertinent to immune response due to infection. Moreover, several recent reports implicate the endotoxin hypothesis driving neurodegeneration [74,75,76]. Whether the moderate dose of peripheral LPS used in our study leads to direct TLR4 stimulation within the brain parenchyma or induces a cytokine storm to trigger brain inflammation, the result in our study is that microglia become highly activated and the brain is flooded with pro-inflammatory molecules that persist after 24 h in IL-10-deficient mice. Our data is consistent with a model (Fig. 7), whereby IL-10 has an important role in limiting an ongoing inflammatory response leading to tau hyperphosphorylation relevant to AD.
Our study shows that IL-10 deficiency is sufficient to promote tau hyperphosphorylation and dysregulated neuroinflammation in the context of an acute peripheral inflammatory insult. Genetic deletion of Il10 promoted enhanced pro-inflammatory cytokine expression, activated microglial morphology, and evidence of neuronal loss. Exacerbated neuroinflammation in the IL-10-deficient environment corresponded with increased tau-kinase p38 MAPK activation and significantly increased tau phosphorylation. These data support the significance of IL-10 in modulating pro-inflammatory microglial activation, dysregulated cytokine production, and hyperphosphorylation of AD-relevant tau epitopes.
Availability of data and materials
The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.
Central nervous system
Glyceraldehyde 3-phosphate dehydrogenase
Ionized calcium-binding adapter molecule 1
Integrated density value
- Il10 −/− :
Level of detection
Microtubule-associated protein tau
Mild cognitive impairment
Mini-mental state exams
Meso Scale Discovery multiplex
Peripheral blood mononuclear cell
p38 mitogen-activated protein kinase
p38 mitogen-activated protein kinase type α
Single nucleotide polymorphism
Suppressor of cytokine signaling
Toll-like receptor 4
Triggering receptor expressed on myeloid cells 2
Tumor necrosis factor α
Terminal deoxynucleotidyl transferase dUTP nick end labeling
Lee G, Leugers CJ. Tau and tauopathies. Prog Mol Biol Transl. 2012;107:263–93. https://doi.org/10.1016/B978-0-12-385883-2.00004-7.
Morris M, Maeda S, Vossel K, Mucke L. The many faces of tau. Neuron. 2011;70(3):410–26. https://doi.org/10.1016/j.neuron.2011.04.009.
Buée L, Bussière T, Buée-Scherrer V, Delacourte A, Hof PR. Tau protein isoforms, phosphorylation and role in neurodegenerative disorders11These authors contributed equally to this work. Brain Res Rev. 2000;33(1):95–130. https://doi.org/10.1016/S0165-0173(00)00019-9.
Lee V, Goedert M, Trojanowski JQ. Neurodegenerative tauopathies. Annu Rev Neurosci. 2001;24(1):1121–59. https://doi.org/10.1146/annurev.neuro.24.1.1121.
O’Leary JC, Li Q, Marinec P, Blair LJ, Congdon EE, Johnson AG, et al. Phenothiazine-mediated rescue of cognition in tau transgenic mice requires neuroprotection and reduced soluble tau burden. Mol Neurodegener. 2010;5(1):45. https://doi.org/10.1186/1750-1326-5-45.
Nelson PT, Alafuzoff I, Bigio EH, Bouras C, Braak H, Cairns NJ, et al. Correlation of Alzheimer disease neuropathologic changes with cognitive status: a review of the literature. J Neuropathol Exp Neurol. 2012;71(5):362–81. https://doi.org/10.1097/NEN.0b013e31825018f7.
Schöll M, Lockhart SN, Schonhaut DR, O’Neil JP, Janabi M, Ossenkoppele R, et al. PET Imaging of tau deposition in the aging human brain. Neuron. 2016;89(5):971–82. https://doi.org/10.1016/j.neuron.2016.01.028.
Heneka MT, Carson MJ, Khoury J, Landreth GE, Brosseron F, Feinstein DL, et al. Neuroinflammation in Alzheimer’s disease. Lancet Neurol. 2015;14(4):388–405. https://doi.org/10.1016/S1474-4422(15)70016-5.
Ising C, Venegas C, Zhang S, Scheiblich H, Schmidt SV, Vieira-Saecker A, et al. NLRP3 inflammasome activation drives tau pathology. Nature. 2019;575(7784):669–73. https://doi.org/10.1038/s41586-019-1769-z.
Glass CK, Saijo K, Winner B, Marchetto MC, Gage FH. Mechanisms underlying inflammation in neurodegeneration. Cell. 2010;140(6):918–34. https://doi.org/10.1016/j.cell.2010.02.016.
Wyss-Coray T, Rogers J. Inflammation in Alzheimer disease—a brief review of the basic science and clinical literature. Csh Perspect Med. 2012;2(1):a006346.
Maphis N, Xu G, Kokiko-Cochran ON, Jiang S, Cardona A, Ransohoff RM, et al. Reactive microglia drive tau pathology and contribute to the spreading of pathological tau in the brain. Brain J Neurol. 2015;138(Pt 6):1738–55. https://doi.org/10.1093/brain/awv081.
Moore KW, de Malefyt R, Coffman RL, O’Garra A. Interleukin-10 and the interleukin-10 receptor. Annu Rev Immunol. 2001;19(1):683–765. https://doi.org/10.1146/annurev.immunol.19.1.683.
Strle K, Zhou J-H, Shen W-H, Broussard SR, Johnson RW, Freund GG, et al. lnterleukin-10 in the Brain. Crit Rev Immunol. 2001;21(5):23.
Ledeboer A, Brevé JJ, Wierinckx A, Jagt S, Bristow AF, Leysen JE, et al. Expression and regulation of interleukin-10 and interleukin-10 receptor in rat astroglial and microglial cells. Eur J Neurosci. 2002;16(7):1175–85. https://doi.org/10.1046/j.1460-9568.2002.02200.x.
Shemer A, Scheyltjens I, Frumer GR, Kim J-S, Grozovski J, Ayanaw S, et al. Interleukin-10 prevents pathological microglia hyperactivation following peripheral endotoxin challenge. Immunity. 2020;53(5):1033–1049.e7. https://doi.org/10.1016/j.immuni.2020.09.018.
Saraiva M, O’Garra A. The regulation of IL-10 production by immune cells. Nat Rev Immunol. 2010;10(3):170–81. https://doi.org/10.1038/nri2711.
Strle K, Zhou J-H, Broussard SR, Venters HD, Johnson RW, Freund GG, et al. IL-10 promotes survival of microglia without activating Akt. J Neuroimmunol. 2002;122(1–2):9–19. https://doi.org/10.1016/S0165-5728(01)00444-1.
Bai F, Xie C, Yuan Y, Shi Y, Zhang Z. Promoter haplotypes of interleukin-10 gene linked to cortex plasticity in subjects with risk of Alzheimer’s disease. Neuroimage Clin. 2018;17:587–95. https://doi.org/10.1016/j.nicl.2017.11.019.
Lio D, Licastro F, Scola L, Chiappelli M, Grimaldi L, Crivello A, et al. Interleukin-10 promoter polymorphism in sporadic Alzheimer’s disease. Genes Immun. 2003;4(3):234–8. https://doi.org/10.1038/sj.gene.6363964.
Arosio B, Trabattoni D, Galimberti L, Bucciarelli P, Fasano F, Calabresi C, et al. Interleukin-10 and interleukin-6 gene polymorphisms as risk factors for Alzheimer’s disease. Neurobiol Aging. 2004;25(8):1009–15. https://doi.org/10.1016/j.neurobiolaging.2003.10.009.
Zhang Y, Zhang J, Tian C, Xiao Y, Li X, He C, et al. The −1082G/A polymorphism in IL-10 gene is associated with risk of Alzheimer’s disease: a meta-analysis. J Neurol Sci. 2011;303(1–2):133–8. https://doi.org/10.1016/j.jns.2010.12.005.
Michaud J-P, Rivest S. Anti-inflammatory signaling in microglia exacerbates Alzheimer’s disease-related pathology. Neuron. 2015;85(3):450–2. https://doi.org/10.1016/j.neuron.2015.01.021.
Chakrabarty P, Li A, Ceballos-Diaz C, Eddy JA, Funk CC, Moore B, et al. IL-10 alters immunoproteostasis in APP mice, increasing plaque burden and worsening cognitive behavior. Neuron. 2015;85(3):519–33. https://doi.org/10.1016/j.neuron.2014.11.020.
Bhaskar K, Konerth M, Kokiko-Cochran ON, Cardona A, Ransohoff RM, Lamb BT. Regulation of tau pathology by the microglial fractalkine receptor. Neuron. 2010;68(1):19–31. https://doi.org/10.1016/j.neuron.2010.08.023.
Kuhn R, Lohler J, Rennick D, Rajewsky K, Muller W. Interleukin-10-deficient mice develop chronic enterocolitis. Cell. 1993;75(2):263–74. https://doi.org/10.1016/0092-8674(93)80068-P.
Bemiller SM, Maphis NM, Formica SV, Wilson GN, Miller CM, Xu G, et al. Genetically enhancing the expression of chemokine domain of CX3CL1 fails to prevent tau pathology in mouse models of tauopathy. J Neuroinflammation. 2018;15(1):278. https://doi.org/10.1186/s12974-018-1310-6.
Maxwell JR, Denson JL, Joste NE, Robinson S, Jantzie LL. Combined in utero hypoxia-ischemia and lipopolysaccharide administration in rats induces chorioamnionitis and a fetal inflammatory response syndrome. Placenta. 2015;36(12):1378–84. https://doi.org/10.1016/j.placenta.2015.10.009.
Yellowhair TR, Noor S, Maxwell JR, Anstine CV, Oppong AY, Robinson S, et al. Preclinical chorioamnionitis dysregulates CXCL1/CXCR2 signaling throughout the placental-fetal-brain axis. Exp Neurol. 2018;301(Pt B):110–9.
Jantzie LL, Maxwell JR, Newville JC, Yellowhair TR, Kitase Y, Madurai N, et al. Prenatal opioid exposure: the next neonatal neuroinflammatory disease. Brain Behav Immun. 2019;84:45–58.
Young K, Morrison H. Quantifying microglia morphology from photomicrographs of immunohistochemistry prepared tissue using ImageJ. J Vis Exp Jove. 2018;136:57648.
Beaudoin GMJ, Lee S-H, Singh D, Yuan Y, Ng Y-G, Reichardt LF, et al. Culturing pyramidal neurons from the early postnatal mouse hippocampus and cortex. Nat Protoc. 2012;7(9):1741–54. https://doi.org/10.1038/nprot.2012.099.
Mattsson N, Schöll M, Strandberg O, Smith R, Palmqvist S, Insel PS, et al. 18F-AV-1451 and CSF T-tau and P-tau as biomarkers in Alzheimer's disease. Embo Mol Med. 2017;9(9):1212–23. https://doi.org/10.15252/emmm.201707809.
Barthélemy NR, Li Y, Joseph-Mathurin N, Gordon BA, Hassenstab J, Benzinger Tammie LS, et al. A soluble phosphorylated tau signature links tau, amyloid and the evolution of stages of dominantly inherited Alzheimer’s disease. Nat Med. 2020;26(3):398–407. https://doi.org/10.1038/s41591-020-0781-z.
Biernat J, Mandelkow EM, Schröter C, Lichtenberg-Kraag B, Steiner B, Berling B, et al. The switch of tau protein to an Alzheimer-like state includes the phosphorylation of two serine-proline motifs upstream of the microtubule binding region. EMBO J. 1992;11(4):1593–7. https://doi.org/10.1002/j.1460-2075.1992.tb05204.x.
Goedert M, Jakes R, Vanmechelen E. Monoclonal antibody AT8 recognises tau protein phosphorylated at both serine 202 and threonine 205. Neurosci Lett. 1995;189(3):167–70. https://doi.org/10.1016/0304-3940(95)11484-E.
Despres C, Byrne C, Qi H, Cantrelle F-X, Huvent I, Chambraud B, et al. Identification of the Tau phosphorylation pattern that drives its aggregation. Proc Nat Acad Sci. 2017;114(34):9080–5. https://doi.org/10.1073/pnas.1708448114.
Hauw J-J, Verny M, Delaère P, Cervera P, He Y, Duyckaerts C. Constant neurofibrillary changes in the neocortex in progressive supranuclear palsy. Basic differences with Alzheimer’s disease and aging. Neurosci Lett. 1990;119(2):182–6. https://doi.org/10.1016/0304-3940(90)90829-X.
Yamada T, McGeer PL, McGeer EG. Appearance of paired nucleated, Tau-positive glia in patients with progressive supranuclear palsy brain tissue. Neurosci Lett. 1992;135(1):99–102. https://doi.org/10.1016/0304-3940(92)90145-W.
Komori T. Tau-positive dial Inclusions in progressive supranuclear palsy, corticobasal degeneration and Pick’s disease. Brain Pathol. 1999;9(4):663–79. https://doi.org/10.1111/j.1750-3639.1999.tb00549.x.
Bachstetter AD, Eldik LJV. The p38 MAP kinase family as regulators of proinflammatory cytokine production in degenerative diseases of the CNS. Aging Dis. 2010;1(3):199–211.
Reynolds CH, Nebreda AR, Gibb GM, Utton MA, Anderton BH. Reactivating kinase/p38 phosphorylates τ protein in vitro. J Neurochem. 1997;69(1):191–8. https://doi.org/10.1046/j.1471-4159.1997.69010191.x.
Reynolds CH, Betts JC, Blackstock WP, Nebreda AR, Anderton BH. Phosphorylation sites on tau identified by nanoelectrospray mass spectrometry. J Neurochem. 2000;74(4):1587–95. https://doi.org/10.1046/j.1471-4159.2000.0741587.x.
Zhu X, Rottkamp CA, Boux H, Takeda A, Perry G, Smith MA. Activation of p38 kinase links tau phosphorylation, oxidative stress, and cell cycle-related events in Alzheimer disease. J Neuropathol Exp Neurol. 2000;59(10):880–8. https://doi.org/10.1093/jnen/59.10.880.
Sun A, Liu M, Nguyen XV, Bing G. P38 MAP kinase is activated at early stages in Alzheimer’s disease brain. Exp Neurol. 2003;183(2):394–405. https://doi.org/10.1016/S0014-4886(03)00180-8.
Maphis N, Jiang S, Xu G, Kokiko-Cochran ON, Roy SM, Eldik LJV, et al. Selective suppression of the α isoform of p38 MAPK rescues late-stage tau pathology. Alzheimers Res Ther. 2016;8(1):54. https://doi.org/10.1186/s13195-016-0221-y.
Arosio B, Mastronardi L, Vergani C, Annoni G. Intereleukin-10 promoter polymorphism in mild cognitive impairment and in its clinical evolution. Int J Alzheimers Dis. 2010;2010:854527.
Scassellati C, Zanardini R, Squitti R, Bocchio-Chiavetto L, Bonvicini C, Binetti G, et al. Promoter haplotypes of interleukin-10 gene and sporadic Alzheimer’s disease. Neurosci Lett. 2004;356(2):119–22. https://doi.org/10.1016/j.neulet.2003.11.033.
Turner DM, Williams DM, Sankaran D, Lazarus M, Sinnott PJ, Hutchinson IV. An investigation of polymorphism in the interleukin-10 gene promoter. Eur J Immunogenet. 1997;24(1):1–8. https://doi.org/10.1111/j.1365-2370.1997.tb00001.x.
Asselineau D, Benlhassan K, Arosio B, Mari D, Ferri E, Casati M, et al. Interleukin-10 production in response to amyloid-β differs between slow and fast decliners in patients with Alzheimer’s disease. J Alzheimer’s Dis Jad. 2015;46(4):837–42. https://doi.org/10.3233/JAD-142832.
Kunkle BW, Grenier-Boley B, Sims R, Bis JC, Damotte V, Naj AC, et al. Genetic meta-analysis of diagnosed Alzheimer’s disease identifies new risk loci and implicates Aβ, tau, immunity and lipid processing. Nat Genet. 2019;51(3):414–30. https://doi.org/10.1038/s41588-019-0358-2.
Jansen IE, Savage JE, Watanabe K, Bryois J, Williams DM, Steinberg S, et al. Genome-wide meta-analysis identifies new loci and functional pathways influencing Alzheimer’s disease risk. Nat Genet. 2019;51(3):404–13. https://doi.org/10.1038/s41588-018-0311-9.
Yoshiyama Y, Higuchi M, Zhang B, Huang S-M, Iwata N, Saido TC, et al. Synapse loss and microglial activation precede tangles in a p301s tauopathy mouse model. Neuron. 2007;53(3):337–51. https://doi.org/10.1016/j.neuron.2007.01.010.
Almolda B, de Labra C, Barrera I, Gruart A, Delgado-Garcia JM, Villacampa N, et al. Alterations in microglial phenotype and hippocampal neuronal function in transgenic mice with astrocyte-targeted production of interleukin-10. Brain Behav Immun. 2015;45:80–97. https://doi.org/10.1016/j.bbi.2014.10.015.
Laffer B, Bauer D, Wasmuth S, Busch M, Jalilvand T, Thanos S, et al. Loss of IL-10 promotes differentiation of microglia to a M1 phenotype. Front Cell Neurosci. 2019;13:430. https://doi.org/10.3389/fncel.2019.00430.
Guillot-Sestier M-V, Doty KR, Gate D, Rodriguez J, Leung BP, Rezai-Zadeh K, et al. Il10 deficiency rebalances innate immunity to mitigate Alzheimer-like pathology. Neuron. 2015;85(3):534–48. https://doi.org/10.1016/j.neuron.2014.12.068.
Yi S, Jiang X, Tang X, Li Y, Xiao C, Zhang J, et al. IL-4 and IL-10 promotes phagocytic activity of microglia by up-regulation of TREM2. Cytotechnology. 2020:1–14.
Heneka MT, Kummer MP, Stutz A, Delekate A, Schwartz S, Vieira-Saecker A, et al. NLRP3 is activated in Alzheimer’s disease and contributes to pathology in APP/PS1 mice. Nature. 2013;493(7434):674–8. https://doi.org/10.1038/nature11729.
Tarkowski E, Andreasen N, Tarkowski A, Blennow K. Intrathecal inflammation precedes development of Alzheimer’s disease. J Neurol Neurosurg Psychiatry. 2003;74(9):1200–5. https://doi.org/10.1136/jnnp.74.9.1200.
Taipa R, SP das Neves, Sousa AL, Fernandes J, Pinto C, Correia AP, et al. Proinflammatory and anti-inflammatory cytokines in the CSF of patients with Alzheimer’s disease and their correlation with cognitive decline. Neurobiol Aging. 2019;76:125–32. https://doi.org/10.1016/j.neurobiolaging.2018.12.019.
Sabat R, Grütz G, Warszawska K, Kirsch S, Witte E, Wolk K, et al. Biology of interleukin-10. Cytokine Growth F R. 2010;21(5):331–44. https://doi.org/10.1016/j.cytogfr.2010.09.002.
Cianciulli A, Dragone T, Calvello R, Porro C, Trotta T, Lofrumento D, et al. IL-10 plays a pivotal role in anti-inflammatory effects of resveratrol in activated microglia cells. Int Immunopharmacol. 2015;24(2):369–76. https://doi.org/10.1016/j.intimp.2014.12.035.
Hammer M, Mages J, Dietrich H, Schmitz F, Striebel F, Murray PJ, et al. Control of dual-specificity phosphatase-1 expression in activated macrophages by IL-10. Eur J Immunol. 2005;35(10):2991–3001. https://doi.org/10.1002/eji.200526192.
Kim C, Sano Y, Todorova K, Carlson BA, Arpa L, Celada A, et al. The kinase p38α serves cell type–specific inflammatory functions in skin injury and coordinates pro- and anti-inflammatory gene expression. Nat Immunol. 2008;9(9):1019–27. https://doi.org/10.1038/ni.1640.
Ledeboer A, Brevé J, Poole S, Tilders F, Dam A. Interleukin-10, interleukin-4, and transforming growth factor-β differentially regulate lipopolysaccharide-induced production of pro-inflammatory cytokines and nitric oxide in co-cultures of rat astroglial and microglial cells. Glia. 2000;30(2):134–42. https://doi.org/10.1002/(SICI)1098-1136(200004)30:2<134::AID-GLIA3>3.0.CO;2-3.
Ledeboer A, Binnekade R, Brevé JJ, Bol JG, Tilders FJ, Dam A-M. Site-specific modulation of LPS-induced fever and interleukin-1β expression in rats by interleukin-10. Am J Physiol Reg Integr Comp Physiol. 2002;282(6):R1762–72. https://doi.org/10.1152/ajpregu.00766.2001.
Sanz JM, Virgilio FD. Kinetics and Mechanism of ATP-Dependent IL-1β release from microglial cells. J Immunol. 2000;164(9):4893–8. https://doi.org/10.4049/jimmunol.164.9.4893.
Licastro F, Pedrini S, Caputo L, Annoni G, Davis LJ, Ferri C, et al. Increased plasma levels of interleukin-1, interleukin-6 and α-1-antichymotrypsin in patients with Alzheimer’s disease: peripheral inflammation or signals from the brain? J Neuroimmunol. 2000;103(1):97–102. https://doi.org/10.1016/S0165-5728(99)00226-X.
Licastro F, Chiappelli M. Brain immune responses cognitive decline and dementia: relationship with phenotype expression and genetic background. Mech Ageing Dev. 2003;124(4):539–48. https://doi.org/10.1016/S0047-6374(03)00034-4.
Quintanilla RA, Orellana DI, González-Billault C, Maccioni RB. Interleukin-6 induces Alzheimer-type phosphorylation of tau protein by deregulating the cdk5/p35 pathway. Exp Cell Res. 2004;295(1):245–57. https://doi.org/10.1016/j.yexcr.2004.01.002.
Fassbender K, Walter S, Kühl S, Landmann R, Ishii K, Bertsch T, et al. The LPS receptor (CD14) links innate immunity with Alzheimer’s disease. FASEB J. 2004;18(1):203–5. https://doi.org/10.1096/fj.03-0364fje.
Walter S, Letiembre M, Liu Y, Heine H, Penke B, Hao W, et al. Role of the toll-like receptor 4 in neuroinflammation in Alzheimer’s disease. Cell Physiol Biochem. 2007;20(6):947–56. https://doi.org/10.1159/000110455.
Kigerl KA, de Rivero Vaccari JP, Dietrich WD, Popovich PG, Keane RW. Pattern recognition receptors and central nervous system repair. Exp Neurol. 2014;258:5–16. https://doi.org/10.1016/j.expneurol.2014.01.001.
Zhao Y, Cong L, Jaber V, Lukiw WJ. Microbiome-derived lipopolysaccharide enriched in the perinuclear region of Alzheimer’s disease brain. Front Immunol. 2017;8:1064. https://doi.org/10.3389/fimmu.2017.01064.
Brown GC. The endotoxin hypothesis of neurodegeneration. J Neuroinflammation. 2019;16(1):180. https://doi.org/10.1186/s12974-019-1564-7.
Patil KR, Mahajan UB, Unger BS, Goyal SN, Belemkar S, Surana SJ, et al. Animal models of inflammation for screening of anti-inflammatory drugs: implications for the discovery and development of phytopharmaceuticals. Int J Mol Sci. 2019;20(18):4367. https://doi.org/10.3390/ijms20184367.
We thank Dr. Erin Milligan for providing the initial set of Il10−/− mice for preliminary data. Ms. Tracylyn Yellowhair for providing professional support with MSD experiments. Mr. Akshay Warrier for laboratory assistance as a trainee. Dr. Jason Weick and Dr. Praveen Chander for primary neuronal culture training. Dr. Sharina Desai for training at the AIM CoBRE. Dr. Michael Paffett for training and assistance at the UNM Cancer Center Fluorescence Microscopy Shared Resource facility.
This work was primarily funded by the Infectious Disease and Inflammation Program pre-doctoral T32 training grant, NIH/NIAID T32AI007538 (to LW). Additional support was from R01NS083704 and 2RF1NS083704-05A1 (to KB), University of New Mexico Stephanie Ruby Predoctoral Travel Award and Brain & Behavioral Health Institute mini-grant (to LW), and Autophagy Inflammation and Metabolism (AIM) Center for Biomedical Research Excellence (CoBRE) NIH grant P20GM121176 (to Dr. Vojo Deretic). This research made use of the Fluorescence Microscopy and Cell Imaging Shared Resource which is partially supported by UNM Comprehensive Cancer Center Support Grant NCI P30CA118100.
Ethics approval and consent to participate
All animal experiments performed in this study were in accordance with the ethical standards of the Institutional Animal Care and Use Committee at the University of New Mexico.
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.
About this article
Cite this article
Weston, L.L., Jiang, S., Chisholm, D. et al. Interleukin-10 deficiency exacerbates inflammation-induced tau pathology. J Neuroinflammation 18, 161 (2021). https://doi.org/10.1186/s12974-021-02211-1
- Alzheimer’s disease