Adenosine triggers early astrocyte reactivity that provokes microglial responses and drives the pathogenesis of sepsis-associated encephalopathy in mice

Guo, Qilin; Gobbo, Davide; Zhao, Na; Zhang, Hong; Awuku, Nana-Oye; Liu, Qing; Fang, Li-Pao; Gampfer, Tanja M.; Meyer, Markus R.; Zhao, Renping; Bai, Xianshu; Bian, Shan; Scheller, Anja; Kirchhoff, Frank; Huang, Wenhui

doi:10.1038/s41467-024-50466-y

Download PDF

Article
Open access
Published: 27 July 2024

Adenosine triggers early astrocyte reactivity that provokes microglial responses and drives the pathogenesis of sepsis-associated encephalopathy in mice

Nature Communications volume 15, Article number: 6340 (2024) Cite this article

3323 Accesses
3 Citations
8 Altmetric
Metrics details

Subjects

An Author Correction to this article was published on 18 September 2024

This article has been updated

Abstract

Molecular pathways mediating systemic inflammation entering the brain parenchyma to induce sepsis-associated encephalopathy (SAE) remain elusive. Here, we report that in mice during the first 6 hours of peripheral lipopolysaccharide (LPS)-evoked systemic inflammation (6 hpi), the plasma level of adenosine quickly increased and enhanced the tone of central extracellular adenosine which then provoked neuroinflammation by triggering early astrocyte reactivity. Specific ablation of astrocytic Gi protein-coupled A1 adenosine receptors (A1ARs) prevented this early reactivity and reduced the levels of inflammatory factors (e.g., CCL2, CCL5, and CXCL1) in astrocytes, thereby alleviating microglial reaction, ameliorating blood-brain barrier disruption, peripheral immune cell infiltration, neuronal dysfunction, and depression-like behaviour in the mice. Chemogenetic stimulation of Gi signaling in A1AR-deficent astrocytes at 2 and 4 hpi of LPS injection could restore neuroinflammation and depression-like behaviour, highlighting astrocytes rather than microglia as early drivers of neuroinflammation. Our results identify early astrocyte reactivity towards peripheral and central levels of adenosine as an important pathway driving SAE and highlight the potential of targeting A1ARs for therapeutic intervention.

Innate Immune Functions of Astrocytes are Dependent Upon Tumor Necrosis Factor-Alpha

Article Open access 27 April 2020

Reactive astrocytes transduce inflammation in a blood-brain barrier model through a TNF-STAT3 signaling axis and secretion of alpha 1-antichymotrypsin

Article Open access 02 November 2022

Artemisinin improves neurocognitive deficits associated with sepsis by activating the AMPK axis in microglia

Article 23 March 2021

Introduction

Severe systemic inflammation caused by infections or injuries can eventually deteriorate to a life-threatening status called sepsis¹. Such systemic inflammation also induces impaired functions of the central nervous system (CNS), one of the first affected organs in sepsis, leading to so-called sepsis-associated encephalopathy (SAE)². Neuroinflammation is a hallmark of SAE, contributing to blood-brain barrier (BBB) damage, altered neuronal activity, and sickness/depression-like behaviour^3,4. Immune signals mediating systemic inflammation were shown to evoke rapid inflammatory responses firstly in components of the BBB (i.e., endothelial cells and pericytes of the brain vasculature) 1-2 h after the systemic inflammation challenge, subsequently releasing inflammatory mediators such as prostaglandin E2 or the chemokine (C-C motif) ligand 2 (CCL2, also referred to as monocyte chemoattractant protein 1, MCP1) and further potentiating neuroinflammation as well as aberrant neuronal activity^3,5,6,7. However, astrocytes were usually considered as targets of reactive microglia after a systemic inflammation challenge rather than early drivers of neuroinflammation themselves, which is counterintuitive concerning their anatomic positions as gatekeepers of the BBB easily receiving signals from the circulation.

Previous studies focused on augmented proinflammatory cytokines (e.g., TNFα, IL-1α and β, and IL-6) of the blood as immune signals which induce inflammatory responses in the CNS³. In addition to cytokines, different purine metabolites such as ATP and adenosine can be found at elevated blood levels after a systemic inflammation challenge^8,9,10,11. However, the roles of purinergic signaling, if any, in affecting initiation and progression of SAE are largely undetermined. In the present study, we examined whether and how extracellular adenosine, the end-product of ATP hydrolysis, could regulate neuroinflammation using a well-established mouse model of SAE in which sepsis is induced by peripheral (intraperitoneal, i.p.) injection of the endotoxin lipopolysaccharide (LPS)^5,12,13,14. We detected rapid increases of extracellular adenosine levels in the blood and the brain shortly after the LPS injection which were followed by neuroinflammatory response of astrocytes, microglia, and neurons in the CNS. We further showed the first in vivo evidence that elevated plasma adenosine signal could pass the BBB to enhance the central adenosine levels. Direct i.p. injection of adenosine or its analogues (i.e., 5′-N-ethylcarboxamide adenosine, NECA; and N6-cyclopentyladenosine, CPA) could induce an upregulation of several proinflammatory factors in the brain, which could be prevented by specific ablation of adenosine A1 receptors (A1ARs) in astrocytes rather than in pericytes, oligodendrocyte precursor cells or microglia, suggesting adenosine as an inflammatory mediator between the body and the CNS via triggering astrocyte reactivity. Comprehensive analyses of mice with inducible and astrocyte-specific A1AR conditional knockout (cKO) mice in the LPS-induced sepsis model further revealed that adenosine triggers astrocyte reactivity via A1ARs which provokes the inflammatory response of microglia at the early phase of systemic inflammation, driving the following pathogenesis of SAE by disrupting the BBB integrity, generating neuronal dysfunction as well as depression-like behaviour of the septic mice.

So far four subtypes of adenosine receptors (i.e., A1, A2a, A2b, A3) have been discovered. However, most previous studies characterizing the neuroimmunological functions of adenosine focused on A2 and A3 AR signaling. Still, our knowledge on the role of A1ARs in regulating neuroinflammation remained scarce^15,16,17. Here, we unveil an important pathway employing adenosine as signaling molecule that mediates systemic inflammation to induce neuroinflammation by triggering early astrocyte reactivity via A1AR signaling. Moreover, we provide evidence that early reactive astrocytes act as drivers of neuroinflammation rather than being the targets of reactive microglia in SAE.

Results

Systemic inflammation increases adenosine levels in the blood and brain

Peripheral administration of a high dose of LPS (such as 5 mg/kg, therefore 1 mg/kg is referred to as low dose in this study) is a widely used method to induce septic systemic inflammation in mice^5,12,14. Sepsis is known to increase plasma adenosine levels in patients or volunteers injected with low doses of LPS^8,10. In the mouse model, we also found elevated levels of plasma adenosine at 2 hours post injection (hpi) of LPS, which peaked at 6 hpi, and subsequently dropped to baseline level at 12 and 24 hpi (Fig. 1a, b). Previous studies suggested that systemic inflammation could disrupt BBB integrity^4,18 and adenosine analogues acting on endothelial A1 and A2a ARs result in the opening of the BBB¹⁹. We also observed that peripheral administration of adenosine itself could increase BBB permeability as assessed by Evans blue (EB) extravasation experiments (Fig. 1c). To further correlate adenosine increase with BBB disruption in systemic inflammation, we performed EB extravasation experiments to study the dynamic changes of BBB integrity after LPS injection. Mice were injected i.v. with EB two hours prior to each analysis time point (Fig. 1a). Intriguingly, our experiments detected BBB disruption already at 2 hpi, which, similar to adenosine changes in the blood, reached the peak at 6 hpi and decreased at 12 and 24 hpi (Fig. 1d). Furthermore, it has been shown that a peripheral injection of LPS could activate various glial cells and pericytes as well as several cytokines in the brain within 24 hours^5,6,14. In our experiments, we also observed enhanced expression of genes related to inflammation (e.g., Ccl2, Ccl5, Cxcl1, Cxcl10, Tnf, Il6, Il1a, and Il1b), astrocyte (Gfap and Lcn2) or microglia reaction (Itgam) in the mouse cortex. Peaks of expression of the inflammation-related proteins reached between 2 and 6 hours post injection (Supplementary Fig. 1a–c), concomitant with a plasma adenosine increase and a BBB disruption, as signs of systemic inflammation.

**Fig. 1: Peripheral LPS challenges increase adenosine levels in the blood and brain.**

To investigate whether systemic inflammation could also evoke extracellular adenosine level in the brain parenchyma, we performed in vivo 2-photon laser-scanning microscopy (2P-LSM) of a novel genetically encoded G protein-coupled receptor (GPCR)-activation-based (GRAB) sensor for adenosine (GRAB_Ado1.0) (Fig. 1e)²⁰ expressed in astrocytes in the somatosensory cortex. We detected increased fluorescence intensities (F.I.) of GRAB_Ado1.0 already at 2 hpi, reaching plateau levels at 6 hpi (Fig. 1f, g), suggesting that LPS-induced systemic inflammation could increase the extracellular adenosine level in the brain, in agreement with prior studies using intracerebral biosensor recordings in rat²¹. Next, we examined whether peripheral adenosine in the blood could directly induce elevation of extracellular adenosine level in the brain. We injected i.p. adenosine (20 mg/kg) supplemented with sulforhodamine 101 (SR101, red fluorescence) to GRAB_Ado1.0-expressing mice during 2P-LSM live imaging (Fig. 1h; Supplementary Movie 2). We were able to detect increased GRAB_Ado1.0 F.I. after the adenosine injection, which is concomitant with the increase of SR101 F.I. in the blood vessels, while injection of SR101 alone could not increase the GRAB_Ado1.0 F.I. (Fig. 1i, j; Supplementary Movie 1). In addition, we observed a dose-dependent increase of GRAB_Ado1.0 F.I. when we injected different doses of adenosine (5−20 mg/kg, Fig. 1k), indicating that increased peripheral adenosine can directly enhance the extracellular adenosine level in the brain. Taken together, we determined the dynamic changes of adenosine levels in the blood and somatosensory cortex post-peripheral LPS challenge. Although the potential sources of the increased extracellular adenosine in the brain after LPS treatment remain unidentified and there is a lack of evidence from previous studies showing adenosine could pass the BBB under normal conditions, our current results strongly suggest that peripheral LPS injection induced a rapid increase of plasma adenosine which may contribute to the elevated extracellular adenosine level in the brain as well as a rapid neuroinflammatory response in the early phase of the systemic inflammation with a disruption of BBB function.

Peripheral adenosine administration induces astrocyte reactivity and neuroinflammation via A1ARs

To evaluate if adenosine could evoke a neuroinflammatory response, we injected adenosine (i.p., 5 mg/kg, six times, at one-hour interval) to ‘wild-type’ (wt) control (ctl) mice and analysed gene expression levels in the mouse cerebral cortex by qPCR at 6 h post the first injection (Fig. 2a). We injected adenosine several times due to its short lifetime in the blood (~1 h)²². Intriguingly, Lcn2 (a marker for inflammatory reactive astrocytes)²³ was upregulated (Fig. 2b; Supplementary Fig. 2a) upon adenosine administration. Moreover, several other proinflammatory cytokine/chemokine genes such as, Ccl2, Cxcl1, Il1a and Tnf also rapidly responded to the adenosine application with increased expression level (Fig. 2b; Supplementary Fig. 2a). Because the plasma adenosine level increased rapidly with the LPS injection and peaked at 6 hpi, we injected NECA (1 mg/kg, a non-selective adenosine analogue, half-life = ~5 h)^19,24 to ctl mice and analysed cytokine expression at 6 hpi (Fig. 2a). We observed that several cytokines such as Cxcl1, Cxcl10, Ccl2, Tnf, Il6 as well as Lcn2 were also upregulated upon NECA treatment (Fig. 2b; Supplementary Fig. 2b). In addition, we injected CPA (1 mg/kg, a selective A1AR agonist, half-life = ~0.5 h) to ctl mice and also detected upregulated cytokines and other proteins related to inflammation/astrocyte activation at 6 hpi (Fig. 2a, b; Supplementary Fig. 2c). Furthermore, when we combined the injection of CPA with a low dose of LPS (1 mg/kg, LPS^low), the expression levels of all tested cytokines or chemokines were strongly augmented compared to mice injected with LPS only (Fig. 2c, Supplementary Fig. 2f). On the other hand, in the cortex of high-dose (5 mg/kg, LPS^high) LPS-challenged mice the administration of DPCPX (1 mg/kg, 8-Cyclopentyl-1,3-dipropylxanthine, a selective A1AR antagonist) inhibited the activation of glial cells and neurons (Supplementary Fig. 2d, e) as well as reduced the expression of several inflammatory factors (e.g., Ccl2, Tnf, Lcn2, Il6, and Cxcl10) (Fig. 2c; Supplementary Fig. 2g). In conclusion, our results strongly suggest that A1AR signaling directly contributes to the induction of neuroinflammation.

**Fig. 2: Peripheral adenosine administration evokes upregulation of inflammation-related genes in the brain.**

Recent transcriptomic studies suggested that A1ARs are the most abundantly expressed ARs in astrocytes^25,26. To determine the contribution of astrocyte-specific A1ARs to adenosine-evoked neuroinflammation, we crossbred GLAST-CreERT2 mice with temporal control of astrocyte-specific gene recombination²⁷ to floxed Adora1 mice²⁸, thereby generating inducible astrocytic Adora1 cKO mice (Fig. 2d) (for simplicity they were termed Adora1 cKO mice afterwards). In addition, we crossbred RiboTag mice²⁹ enabling specific and direct purification of mRNAs (mRNA^RiboTag) from Cre-expressing cells in cerebral cortices to avoid pitfalls inherent to cell-sorting procedures (Supplementary Fig. 3a). We performed qPCR and RNA-seq analysis for Adora1^RiboTag expression to reveal a successful gene excision of Adora1 in cKO mice (Supplementary Fig. 3a–d). In parallel, we used a genetically encoded Ca²⁺ indicator mouse line (Rosa26-LSL-GCaMP3, Rosa26-GCaMP3)³⁰ to study Ca²⁺ activity in astrocytes after tamoxifen administration (Supplementary Fig. 4a). We recorded cortical astrocytic Ca²⁺ signalling from astrocytic Adora1 cKO and ctl mice using ex vivo 2P-LSM before and after the focal application of CPA (1 µM) in the presence of the neuronal activity blocker tetrodotoxin (TTX, 1 µM) (Supplementary Fig. 4b, c). The automatic detection of regions-of-activity (ROAs) was performed as previously described³¹ using the custom-made MATLAB-based tool MSparkles³²) (Supplementary Fig. 4c–e). To note, genetic ablation of astrocytic A1ARs was associated with altered baseline Ca²⁺ activity, including an increased number of Ca²⁺ signals with lower amplitude. In particular, A1AR-deficient astrocytes showed increased occurrence of spatially-defined ROAs with reduced area but smaller signal frequency per ROA (Supplementary Fig. 4f, g). Taken together, these results showed that the removal of astrocytic A1ARs results in the reduction of astrocytic Ca²⁺ signals ex vivo in terms of signal amplitude, spatial extension and signal frequency. On the other hand, CPA application triggered significant increases of astrocytic Ca²⁺ signals in ctl mice which was not detected in astrocytic Adora1 cKO mice, further confirming the functional removal of A1ARs from astrocytes.

Subsequently, we injected NECA or CCPA (0.3 mg/kg, 2-chloro-N6-cyclopentyladenosine, a more selective A1AR agonist) to Adora1 cKO and ctl mice and found that the expression of several upregulated cytokines and chemokines (e.g., Ccl2, Ccl5, Cxcl1, Cxcl10, Il1a, and Tnf) was significantly attenuated in Adora1 cKO mice (Fig. 2e, Supplementary Fig. 2h), which was not observed in mice with specific ablation of Adora1 in microglia (using Cx3CR1-CreERT2 mice)and oligodendrocyte precursor cells/pericytes (using NG2-CreERT2 mice, only Ccl2 was reduced) (Fig. 2d, e; Supplementary Fig. 2j, k). In line with the in vivo observation, application of CCPA to primary astrocytes evoked significant upregulation of several chemokines (e.g., Cxcl1, Cxcl10, Ccl5), whereas CV1808 (a non-selective antagonist of A2AR) did not cause significant expression alterations of all the tested inflammation-related genes (Supplementary Fig. 5a–c). Altogether, these results provided additional evidence that adenosine could trigger neuroinflammatory response via astrocytic A1AR signaling.

A1AR signaling augments inflammatory response of reactive astrocytes in the early phase of systemic inflammation

Upregulation of the immediate early gene Fos family is frequently used to indicate activation of neurons as well as early reactive astrocytes upon pathological stimulation^{33,34,35,36,37}. Furthermore, c-Fos expression can be triggered by GPCR signaling in astrocytes. Therefore, we firstly performed immunohistochemistry of c-Fos combined with the astrocyte marker Sox9 on mouse brain slices to investigate the time course of astrocyte reactivity after LPS (5 mg/kg, and for all the following experiments) injection. We found that the expression of c-Fos in astrocytes of ctl mice was unaltered at 2 hpi but was upregulated at 6 hpi and reduced to basal level at 24 hpi. However, the c-Fos expression in astrocytes in cortex, hippocampus, and striatum was significantly inhibited by the deficiency of A1ARs at 6 hpi, indicating a critical early temporal window of the astrocytic response to a systemic inflammation (Fig. 3a–d). In addition, activation of signal transducer and activator of transcription 3 (STAT3) signaling is an important inducer of inflammatory responses of reactive astrocytes³⁸). To evaluate the astrocyte inflammatory response, we performed immunohistochemistry for the activated form of STAT3 (i.e., phospho-STAT3^Tyr705, p-STAT3). In the brain of ctl and Adora1 cKO mice, we observed that p-STAT3 was almost non-detectable at 0 hpi. However, at 6 hpi the p-STAT3 immunoreactivity could be detected in virtually all Sox9⁺ astrocytes of ctl mice which was significantly reduced in Adora1 cKO mice. At 24 hpi, the p-STAT3 expression level was largely reduced (Fig. 3e–h). These results further suggest that the activation of A1AR signaling promote the inflammatory response of reactive astrocytes which peaks in the early phase of the systemic inflammation.

**Fig. 3: A1AR-deficient astrocytes are less reactive to the peripheral LPS challenge.**

Next, we performed high-throughput RNA-seq to further study the impact of A1AR-mediated reactive astrocyte response to systemic inflammation at molecular level. We used the RiboTag approach to directly purify astrocytic translated mRNA (mRNA^RiboTag) from the cortex for RNA-seq analysis (Supplementary Fig. 6a). We observed that astrocytes from ctl mice strongly responded to the peripheral LPS challenge in terms of dynamically up and down-regulating genes with time after LPS injection, in line with the previous reports¹². However, the overall gene expression in A1AR-deficient astrocytes were much less altered upon the LPS injection at 6 and 24 hpi compared to ctl mice (Fig. 4a; Supplementary Fig. 6b; Supplementary Fig. 7). In total, comparing A1AR-deficient astrocytes to ctl astrocytes, we found 12 (4 up, 8 down) differentially expressed genes (DEGs) at 0 hpi (healthy controls), 185 (38 up, 147 down) DEGs at 6 hpi, and 2643 (1465 up, 1178 down) DEGs at 24 hpi (Supplementary Fig. 6c–e). Further Hierarchical Clustering analysis by K-means classified DEGs into 8 clusters (Fig. 4a; Supplementary Fig. 7). At 6 hpi, 125 genes (cluster 1, 5) were upregulated in ctl mice including cytokines and chemokines (e.g., Ccl2, Ccl5, Ccl9, Cxcl1, Cxcl10, etc.), transcription factors that promote inflammation (e.g., Nfkb1a, Nfkb2, Stat3, etc.), and previously identified marker genes of early responding reactive astrocytes such as interferon-responsive genes (e.g., Ifit1, 2, 3) and genes encoding proteins for antigen presentation (e.g., H2-D1, H2-K1)¹². However, in astrocytes of Adora1 cKO mice the expression of those pro-inflammatory genes was inhibited. Of note, at 6 hpi several immediate early genes (e.g., Fos, Jun, and Junb; cluster 5) were also reactively expressed in ctl astrocytes as previously reported^6,12 and were inhibited in Adora1 cKO astrocytes, in agreement with the c-Fos immunohistochemistry results. Unlike genes in cluster 5 (e.g., Fos, Jun, Junb) that were rapidly down-regulated to baseline level at 24 hpi, on average genes in cluster 1 (e.g., Ccl5, Ccl9, Cxcl10, Stat3) were still expressed at high levels in ctl astrocytes but inhibited in A1AR-deficient astrocytes at 24 hpi. In clusters 2, 4, and 6, 918 genes were slightly dysregulated in both ctl and Adora1 cKO astrocytes at 6 hpi but were either up- (cluster 6) or downregulated (cluster 2 and 4) in ctl astrocytes at 24 hpi. However, the expression of these genes in Adora1 cKO astrocytes appeared to be slightly altered at 24 hpi. By Metascape pathway analysis we found that genes in these clusters are responsible for ‘DNA repair’ (e.g., Fancm, Msh3, Xpa, etc. in cluster 6), ‘neuronal system’ (e.g., Gabrd, Mpdz, etc. in cluster 2), and ‘cell projection assembly’ (e.g., Fnbp11, Tppp, Nek1, etc. in cluster 4). We also observed that many genes defined in previous studies as ‘A1 astrocyte’ (e.g., H2-D1, H2-T23, Gbp2, Iigp1, Psm8, etc.) and ‘A2 astrocyte’ (e.g., Clcf1, Tgm1, Ptx3, etc.) markers were decreased in Adora1 cKO astrocytes at 24 hpi (Supplementary Fig. 6f). Therefore, we assume that this difference in Adora1 cKO mice at 24 hpi could be regarded as the consequence of reduced astrocytic inflammatory response at 6 hpi which may ameliorate the global neuroinflammation afterwards (see below). For example, the GSEA-KEGG pathway analysis indicated that genes involved in astrocytic inflammatory response pathways (e.g., ‘NF-kappa B signaling pathway’, ‘JAK-STAT signaling pathway’, ‘IL-17 signaling pathway, NOD-like receptor signaling pathway’, ‘TNF signaling pathway’, etc.)^39,40 were supressed in Adora1 cKO mice at 6 hpi (Fig. 4b, c). Similarly, GSEA-GO term (biological process, BP) analysis also demonstrated that genes annotated to inflammation-related GO terms (e.g., ‘interleukin-1 production’, ‘toll-like receptor signaling pathway’, ‘receptor signaling via JAK-STAT’, ‘I-kappaB/NF-kappaB signaling’, ‘inflammatory response, cytokine response’, ‘interferon-gamma production’, etc.) were suppressed in A1AR-deficient astrocytes at 6 hpi (Fig. 4d, e). Furthermore, Metascape analysis for upstream transcriptional regulators revealed that the suppressed genes in A1AR-deficient astrocytes at 6 hpi were regulated by transcription factors (e.g., Jun, Nfkb1, Cebpb, Stat3, Fos, etc.) known to regulate downstream proinflammatory pathways of reactive astrocytes (Fig. 4f)^39,40. Taken together, our results demonstrated that in the early phase after a peripheral LPS challenge adenosine triggers via A1ARs the inflammatory response of reactive astrocytes, which may influence the subsequent progression of neuropathology.

**Fig. 4: A1AR activation contributes to the altered transcriptional profile of astrocytes upon peripheral LPS challenge.**

Astrocyte reactivity in the early phase of systemic inflammation boosts global neuroinflammation and microglial reaction

We next examined the impact of astrocytic A1AR signaling on the global inflammatory response of the brain following a systemic inflammation challenge. We measured 111 different cytokines in the cortex of ctl and Adora1 cKO mice using a proteomic profiling assay and observed that most of the inflammation-related proteins in the cortex of ctl mice were upregulated after LPS injection at 6 and 24 hpi. However, in Adora1 cKO mice the levels of several astrocyte specific/related proinflammatory proteins (e.g., CXCL1, CXCL10, ICAM-1, lipocalin- 2 (LCN2), MMP3)⁴⁰ and many other cytokines or chemokines of multiple origins including microglia and astrocytes (e.g., CCL2, CCL5, IL-1α, CXCL2, etc.)⁴¹ were largely reduced after LPS injection (Fig. 5a, b; Supplementary Fig. 9b, c), in line with the astrocytic RNA^RiboTag sequencing results. In addition, the differentially expressed protein, LCN2 (Supplementary Fig. 9a), was chosen for Western blot to further confirm the results from the cytokine array. A similarly reduced inflammatory response pattern was detected in the striatum of Adora1 cKO mice using a small-size (40 cytokines) cytokine array immunodot-blot assay (Fig. 5c, d). These results demonstrate reactive astrocytes upon A1AR activation in the early phase of systemic inflammation exacerbates global neuroinflammation afterwards.

**Fig. 5: Astrocytic A1AR deficiency reduces global neuroinflammation induced by an LPS challenge.**

Microglia and astrocytes are key players in neuroinflammation. Previous studies suggested that astrocyte and microglia interact with each other to modulate neuroinflammation^39,42. Particularly, in the peripheral LPS challenge model, astrocytes can become neurotoxic when triggered by cytokines released by activated microglia¹³. However, these pioneer studies focused on the late phase (after 24 hpi) of the LPS model. Our current results show an adenosine-mediated early response (2–6 hpi) of astrocytes to the LPS challenge that regulate the expression of inflammation-related genes, many of which (e.g., Ccl2, Ccl5, Cxcl1 and Cxcl10) have been shown to trigger the formation of reactive microglia⁴⁰. Therefore, we hypothesized that astrocytes could modulate microglia activation in the initial phase of systemic inflammation rather than just be the effector of reactive microglia. It is known that reactive microglia produce many inflammatory cytokines via the NF-κB signaling pathway⁴¹. Therefore, we first examined the reactivity of microglia in the early phase of the LPS model and detected nuclear translocation of p65 (a co-factor of NF-κB) as an indicator of reactive microglia (Fig. 6a).

**Fig. 6: Astrocytic A1AR deficiency inhibits microglial reaction upon LPS challenge.**

We found that peripheral LPS challenge increased the proportion of nuclear p65⁺ microglia in the cortex of ctl mice from ~13% at 2 hpi to ~90% at 6 hpi and ~30% at 24 hpi, whereas such proportion in Adora1 cKO mice was reduced to ~9%, ~55% and ~17% at 2, 6 and 24 hpi, respectively (Fig. 6a, b). Similarly, in the hippocampus and striatum the nuclear p65⁺ microglia were also reduced proportionally in the Adora1 cKO mice at 6 hpi (Fig. 6c, d). Therefore, our results revealed that a systemic LPS challenge initiates astrocyte activation in the early phase via A1AR signaling to augment reactive microglial inflammatory response. In addition, systemic inflammation challenges can enhance the phagocytosis of microglia which contributes to the depression-like behaviour. Therefore, we quantified the CD68⁺ lysosome volume in microglia to assess the phagocytic ability of microglia in our model (Fig. 6e). We found that the volume of CD68⁺ lysosome (in proportion to microglial volume) in the cortex of ctl mice increased from ~1% at 0 hpi to ~4% at 6 hpi and further increased to ~11% at 24 hpi. However, in Adora1 cKO mice such volume enlargement was significantly inhibited to ~2% and ~5% at 6 and 24 hpi, respectively, indicating the microglial phagocytosis was inhibited by the astrocytic A1AR deficiency (Fig. 6e, f). To further confirm these ameliorated phenotypic alterations of microglia, we analysed microglial morphologies in Adora1 cKO and ctl mice (Fig. 6g) by IMARIS software. In the healthy control group (0 hpi), microglia of Adora1 cKO and ctl mice displayed comparable morphologies. However, 6 or 24 hours after LPS injection microglia in Adora1 cKO mice showed more intersections in the Sholl-analysis, more total process length, and a larger occupied area (Fig. 6g–i), indicating reduced microglial activation in the absence of astrocytic A1AR signaling. In line with the morphological changes, we detected that the gene expression levels of microglial homeostasis markers such as P2ry12 were reduced at 6 hpi in both groups. However, at 24 hpi the P2ry12 expression in Adora1 cKO mice recovered to the healthy level while in ctl mice it was still significantly reduced (Fig. 6j). Taken together, our results demonstrate that A1AR signaling triggers early reactive astrocytes to provoke the pathological phenotype formation of reactive microglia after a systemic inflammation challenge.

Astrocytic A1AR signaling contributes to impaired BBB function and peripheral immune cell infiltration in systemic inflammation

Next, we investigated BBB function-related parameters in Adora1 cKO and ctl mice following a peripheral LPS challenge. Systemic inflammation induces the CCL5-CCR5 axis-dependent migration of microglia to blood vessels, which further impairs the BBB¹⁸. We found that after LPS injection the perivascular microglia in ctl mice increased proportionally from ~35% at 0 hpi to ~50% at 6 and 24 hpi, while the proportion of perivascular microglia in Adora1 cKO mice was only increased from ~35% to ~43% at 6 and ~45% at 24 hpi, indicating a significant reduction (~50%) of newly recruited perivascular microglia in Adora1 cKO mice after peripheral LPS injection (Supplementary Fig. 8a–c), in line with the reduction of CCL5 expression in the cKO mice. To assess the BBB integrity, we injected EB i.v. to mice immediately after the LPS injection and allowed EB to circulate for 24 hours. Afterwards, we measured EB extravasation in brain tissue. We detected less EB in the brain of Adora1 cKO mice than in ctl (~10 vs. 22 µg/g tissue, Supplementary Fig. 8d), indicating less disruption of the BBB in Adora1 cKO mice. Systemic inflammation promotes infiltration of peripheral immune cells into the brain parenchyma, attributable to the disrupted BBB as well as an upregulated expression of chemokines (e.g., CXCL1)⁴³ and extracellular matrix proteins (e.g., ICAM-1)⁴⁴. Therefore, we used flow cytometry to identify different immune cell populations in the brain (Supplementary Fig. 8e). We found that at 6 hpi, the proportions of infiltrated monocytes (CD11b⁺/CD45^low+/Ly6C^neg-/Ly6G^high+; ctl: ~4% vs Adora1 cKO: ~2%), neutrophils (CD11b⁺/CD45^low+/Ly6C^inter+/Ly6G^high+; ctl:~4% vs Adora1 cKO: ~2%), and T cells (CD45⁺/CD3^high+/Ly6G^neg-; ctl: ~4% vs Adora1 cKO: ~2%) were significantly reduced in Adora1 cKO mice among all immune cells (Supplementary Fig. 8f, j). Furthermore, we performed Ly6B immunostaining to detect neutrophils at 24 hpi. We found that the entry of Ly6B⁺ cells into the brain parenchyma was largely reduced 24 hours after the peripheral LPS injection in cKO mice compared to ctl (Supplementary Fig. 8h, i), in line with our current finding of reduced CXCL1 and ICAM-1 expression in Adora1 cKO mice. Taken together, upon a systemic inflammation challenge astrocytic A1AR deficiency inhibited microglial reaction and neuroinflammation which ameliorated the impairment of the BBB and reduced peripheral immune cell infiltration.

A1AR-mediated astrocyte activation promotes aberrant neuronal functions and behavioural deficits in systemic inflammation

Systemic inflammation is also known to alter neuronal hyperactivity. For example, two hours after peripheral administration of LPS, pericytes are triggered to release CCL2, which subsequently determines neuronal hyperactivity⁵. Therefore, we performed c-Fos and NeuN (a neuron marker) double immunostaining and studied neuronal activation after a peripheral LPS challenge. In contrast to astrocytes, we observed that c-Fos expression in cortical neurons in ctl mice gradually increased from 6 hpi to 24 hpi. Although c-Fos expression was still elevated in neurons from Adora1 cKO mice compared with basal levels (0 hpi), it was lower than in ctl mice at 6 and 24 hpi (Fig. 7a, b). Similarly, we detected lower c-Fos levels in hippocampal and in striatal NeuN⁺ neurons of Adora1 cKO mice at 24 hpi (Fig. 7c, d). Thereby, these results further confirm that astrocytic A1ARs contribute to neuronal activation upon the challenge of systemic inflammation.

**Fig. 7: Astrocytic A1AR deficiency prevents neuronal dysfunction and ameliorates depression-like behaviour of the mice after LPS treatment.**

Neuroinflammation induced by systemic endotoxin has been shown to affect neuronal network plasticity in terms of impaired long-term potentiation (LTP)^45,46,47. To study the impact of astrocyte-specific A1AR deficiency on neuronal plasticity following a peripheral LPS challenge, we performed extracellular electrophysiological recordings on acute slices prepared from dorsal hippocampi of Adora1 cKO and ctl mice. Neurons from both groups displayed comparable LTP after PBS injection. However, LTP was impaired after LPS injection in ctl mice at 6 and 24 hpi, whereas it was preserved in cKO mice (Fig. 7e–g). These results indicate that adenosine triggers an astrocytic inflammatory response as a detrimental regulator of neuronal functions after systemic LPS challenge.

Neuroinflammation induced by peripheral LPS administration leads to fatigue, muscle weakness, and other sickness behaviour in mice (e.g., hunched posture, reduced food and water intake, etc.) that peaks between 2 and 6 hpi and gradually wanes. Subsequently, the depression-like behaviour (e.g., reduced locomotion in the open-field test, loss of preference to drink sweetened water, etc.) gradually develops to reach the peak 24 hours later^3,14. Therefore, we performed the open-field test to assess the general exploratory locomotion of mice as a total readout of behavioural deficits at 24 hpi (Fig. 7h). We observed ctl and Adora1 cKO mice injected with PBS performed similarly in the open-field test. As expected, after LPS injection all ctl and Adora1 cKO mice drastically reduced locomotion, whereas Adora1 cKO mice moved longer distances than ctl mice (Fig. 7i, j), suggesting that the deficiency of astrocytic A1ARs could alleviate behavioural deficits induced by systemic inflammation. However, the time spent in the central area, a parameter often used to assess depression/anxiety of mice, was heavily reduced in both groups, though the Adora1 cKO mice showed a tendency of increasing the time. Concerning other aspects of the sickness such as fatigue may influence the interpretation of the time spend in the central area, we used the sucrose-preference test to further specifically evaluate anhedonia, another hallmark of systemic inflammation-induced depression-like behaviour (Fig. 7h). We observed that peripheral LPS challenge could largely abolish the sucrose preference of ctl mice from 24-48 hpi (~45%) which partially recovered to ~60% from 48–72 hpi. However, the sucrose preference of Adora1 cKO mice was only partially impaired to ~65% from 24-48 hpi, and almost fully recovered to the healthy level from 48–72 hpi (~80%), again indicating activation of astrocytic A1ARs contributes to behavioural deficits induced by systemic inflammation (Fig. 7k).

Enhancing Gi signaling in A1AR-deficient astrocytes restored neuroinflammation upon peripheral LPS challenge

A1ARs are G_i/o protein-coupled receptors. Therefore, a weakened Gi signaling can be assumed in astrocytes of cKO mice. The Gi signaling could be artificially rescued using Designer Receptors Exclusively Activated by Designer Drugs (DREADD)-based chemogenetic tool hM4Di upon administration of its specific agonist CNO (clozapine N-oxide). Since previous studies highlighted that reactive microglia in the mouse striatum is a major contributor to depression-like behaviours after peripheral LPS challenge⁴⁸, we stereotactically injected AAV-GFAP-hM4Di-mCherry or AAV-GFAP-tdTomato into the striatum of Adora1 cKO and ctl mice to specifically express hM4Di (indicated by mCherry) or tdTomato (tdT, as control) in astrocytes. To study whether A1AR-mediated astrocyte activation at the early phase of systemic inflammation is crucial to provoke the subsequent neuroinflammation, we injected CNO (2 mg/kg, half-life = ~0.5 h) to AAV-delivered mice to evoke Gi signaling at 2 and 4 h post peripheral LPS challenge (Fig. 8a–c). At 6 hpi, we observed that in the Adora1 cKO mice c-Fos expression was more enhanced in hM4Di-expressing rather than in tdT-expressing astrocytes, indicating that Gi signaling could further activate A1AR-deficient astrocytes post LPS injection (Fig. 8d, e). Concomitantly, we found increased nuclear p65⁺ microglia in the regions with hM4Di-expressing astrocytes compared to tdT-expressing astrocytes in Adora1 cKO mice, suggesting that enhancing astrocytic Gi signaling could promote reactive microglial inflammatory response at the early stage of systemic inflammation (Fig. 8f, g). To assess the long-term effect of activation of Gi signaling in A1AR-deficient astrocytes, we measured the expression of proinflammatory factors in AAV-infected brain regions by cytokine array 24 h post LPS injection. We observed that the expression of the factors (e.g., CCL2, CCL5, CCL3, CXCL1, CXCL2, CXCL10, G-CSF, etc.) inhibited in the tdT-expressing Adora1 cKO mice (compared to tdT-expressing ctl mice) could be enhanced to certain extents in hM4Di-expressing Adora1 cKO mice (Fig. 8h, i). In addition, a similar effect could be detected in the cortex of Adora1 cKO mice with astrocytic hM4Di activation (Supplementary Fig. 9d, e), suggesting a consistent effect of Gi signaling in astrocytes from different brain regions to promote neuroinflammation. These results were in line with our previous pharmacological intervention experiments showing the A1AR antagonist DPCPX treatment could reduce neuroinflammation during the early phase of systemic inflammation (Supplementary Fig. 2d, e). Next, we performed an open-field test and found that the alleviated behavioural deficit in Adora1 cKO mice upon LPS challenge could be exacerbated to the level of ctl mice upon astrocytic Gi signaling activation (Fig. 8j–l). Likewise, we observed ctl mice treated with DPCPX at 2 and 4 hpi showed increased locomotion in the open-field test at 24 hpi, suggesting an ameliorated behavioural deficits (Supplementary Fig. 10a–c). In summary, our results strongly suggest that early astrocyte reaction to A1AR signaling in systemic inflammation plays an important role in promoting neuroinflammation to drive pathogenesis of SAE and targeting A1ARs can be a therapeutic approach for SAE.

**Fig. 8: Activation of Gi signaling in A1AR deficit astrocytes restores the inflammatory response to peripheral LPS challenge.**

Discussion

Adenosine has been widely recognized as a guardian molecule that executes protective function in and outside of the CNS. For example, in the periphery adenosine reduced inflammation by triggering A2a, A2b, and A3 ARs of immune cells (e.g., macrophages, lymphocytes, neutrophils, etc.) as demonstrated, among others, in autoimmune diseases (e.g., rheumatoid arthritis), inflammatory bone loss, intestinal inflammation¹⁶. In the CNS, adenosine is known to trigger pre- and post-synaptic A1ARs to reduce neuronal activity and, thereby, to alleviate epilepsy and pain¹⁶. However, recent studies also suggest that the overproduction of adenosine could enhance neuroinflammation, for example, via microglial A2a AR in Parkinson disease (PD)^15,17. In the current study, we revealed that peripheral administration of adenosine or its analogues can directly trigger inflammatory responses in the brain mediated at least partially by astrocytic A1ARs. Using peripheral LPS challenge, we provide further evidence that systemic inflammation-induced adenosine rise in the brain plays an important role via astrocytic A1AR signaling in exacerbating neuroinflammation to drive the pathogenesis of the SAE. Therefore, like its precursor ATP, adenosine can also behave like a DAMP (damage-associated molecular patterns) molecule for neuroinflammation, possibly in a context-dependent manner.

Adenosine is mainly formed from the sequential ATP metabolism by means of a series of hydrolases, among which the ecto-5’-nucleotidase Nt5e (also known as CD73) performs the last step converting AMP to adenosine^49,50. Under cellular stress conditions, such as inflammation or hypoxia, extracellular ATP/adenosine can drastically increase^51,52. Recent studies using a novel genetically modified ATP sensor (GRAB_ATP1.0) provided direct evidence that extracellular ATP levels in the mouse brain were increased after peripheral LPS challenge¹¹. Therefore, it is conceivable that increased extracellular ATP in the brain may contribute to adenosine elevation as well. Indeed, here we detected elevated extracellular adenosine in the brain parenchyma upon LPS injection employing in vivo 2P-LSM imaging of GRAB_Ado1.0 and this effect lasted at least 24 h post the LPS challenge. In addition, adenosine can be transported by equilibrative nucleoside transporters (ENTs) or can bypass, in virtue of its small size, tight junctions (TJs) of endothelial cells^53,54. Furthermore, adenosine can increase the permeability of the BBB through A1 and A2a ARs in endothelial cells, which facilitate the infiltration of peripheral immune cells (or even bacteria) expressing CD73 into the brain parenchyma^19,24,55,56. To determine whether humoral adenosine could not only open the BBB but also further diffuse into the brain parenchyma, we injected adenosine i.p to mice during the 2P-LSM recording of GRAB_Ado1.0 signals. We were able to detect increasing GRAB_Ado1.0 signals in the brain along with the entry of the peripherally administered adenosine into cerebral blood flow indicated by SR101 in a dose-dependent manner. Although locally generated extracellular adenosine was reported to be quickly eliminated within seconds, previous studies have shown that i.p. injected adenosine could remain in the blood for at least one hour^22,24. Therefore, our 2P-LSM results of adenosine administration strongly suggest that peripherally administered adenosine could either pass through the BBB or trigger endothelial cells to release ATP/adenosine (or both), thereby increasing the extracellular adenosine level in the brain parenchyma. We also demonstrated (as found in septic patients and volunteers receiving LPS injection^8,57) that the plasma level of adenosine was increased by the LPS challenge gradually peaking at 6 hpi, concomitant with the progression of astrocytic c-Fos and p-STAT3 expression, BBB breakdown and sickness behaviour of the mice. Moreover, considering that the BBB integrity was impaired by systemic inflammation, which could permit even more adenosine entry from circulation to the brain parenchyma, it is conceivable that systemic inflammation-increased humoral adenosine adds to locally generated adenosine to affect cells building the BBB (e.g., astrocytes and pericytes) at least during the early phase of systemic inflammation, provoking neuroinflammation.

In line with recent studies¹², our c-Fos and p-STAT3 immunohistochemistry as well as RNA^RiboTag sequencing results revealed that astrocytes reacted rapidly within hours to a systemic inflammation challenge and underwent dynamic transcriptomic changes. Although many molecules such as TNFα, IL-1α from reactive microglia, ATP, NO, etc. have been identified as triggers of astrocyte reactivity⁴⁰, the exact molecules that initiate/boost such fast astrocyte reactivity to systemic inflammation are still undefined⁵⁸. Here, we demonstrated that the removal of A1ARs from astrocytes could largely prevent such fast astrocyte reactivity upon LPS injection. Moreover, adenosine and its analogues were able to elicit a neuroinflammatory response in healthy mice, which was strongly attenuated by lack of astrocytic A1AR. Our results suggest that the formation of reactive astrocytes in the early phase of systemic inflammation requires proinflammatory cytokines from the circulation or other CNS cells, but small molecules from the metabolism could play important roles as well. Here, adenosine is proposed as the first identified small molecule. It triggers the early astrocytic response to systemic inflammation via A1AR signaling.

Astrocytes express a plethora of GPCRs on the plasma membrane to sense the extracellular signal molecules such as glutamate, ATP, and adenosine which induce intracellular Ca²⁺ signals. Previous chemogenetic studies suggested that activation of Gi sigaling in astrocytes leads to Ca²⁺ signal elevation via phospholipase C (PLC) pathway^33,37. In the current study using brain slice recording in Adora1 cKO mice we detected more astrocytic spontaneous Ca²⁺ signals (microdomains) with lower amplitude in the presence of TTX, which led to more ROAs with smaller sizes. Although the intracellular mechanisms attributed to such an observation are not yet clear, these results suggest astrocytes respond to endogenous extracellular adenosine via A1ARs under physiological conditions. Nevertheless, on the other hand, astrocytic-A1AR deficiency does not seem to heavily influence the physiological functions of astrocytes in terms of minor alterations of gene expressions, microglia reactivity, BBB integrity, neuronal plasticity, and general behavioural performance in current tests. However, recent studies revealed that pathological stimuli trigger aberrant Ca²⁺ signaling in astrocytes which promotes their reactivity and increases neuroinflammation^59,60. Therefore, it is conceivable that after LPS injection, the increased extracellular adenosine acting on A1ARs could evoke aberrant astrocytic Ca²⁺ signals, though in vivo Ca²⁺ live imaging will be required to further investigate this scenario. Furthermore, our mRNA^RiboTag sequencing and immunohistochemical results demonstrated that several signaling pathways (e.g., Fos-Jun, JAK-STAT3, MAPK) are involved in regulating the A1AR-mediated inflammatory response of astrocytes. Given that intracellular Ca²⁺ activities were suggested to be involved in the regulation of these signaling pathways^33,37,61,62, we could hypothesize that at the early phase of systemic inflammation A1AR activation-induced aberrant Ca²⁺ signals of astrocytes enhance diverse intracellular signaling pathways to provoke the inflammation response as suggested by the RNA profiling analyses.

Recent transcriptomic studies demonstrated astrocytes and microglia are both fast responders at the early phase of systemic inflammation^6,12,45. Although reactive astrocytes were usually considered as the long-term effector of reactive microglia especially in the systemic inflammation model⁵⁸, whether this is the case for the early astrocyte reactivity is unclear. Our astrocytic RNA^RiboTag sequencing results revealed that astrocytes at 6 hpi were triggered to release a series of inflammatory factors that are known to activate microglia via NF-κB activation, which were largely inhibited upon the ablation of A1AR signaling. Compensating the downstream Gi signaling by DREADD hM4Di strategy in the A1AR-deficient astrocytes before 6 hpi could largely restore the NF-κB activation of microglia and global neuroinflammation. Therefore, we provide evidence that astrocytes at the early phase of systemic inflammation behave more like a booster of reactive microglia. Furthermore, the immune signal from the inflamed circulation was shown to be relayed by cells building the BBB (i.e., endothelial cells and pericytes) to the brain parenchyma^5,6,7. As another major component of the BBB, each astrocyte extends its end-feet to wrap at least one blood vessel⁶³. Our results suggest that, in addition to endothelial cells/pericytes, immune signals mediated by adenosine from the circulation stimulate astrocytes to subsequently enhance microglia reaction at the initial phase of the systemic inflammation. Thereby, reactive microglia may in turn modulate astrocyte reactivity in terms of the temporally changed transcriptome towards the neurotoxic A1-type in the late phase of systemic inflammation (24 hpi). However, such adenosine-regulated reciprocal interactions between astrocytes and microglia needs further investigation in other neuroinflammatory diseases such as multiple sclerosis (MS). In addition, future studies need to determine the dynamics of the interactome between astrocytes and microglia (and other inflammation-related cells such oligodendrocyte precursor cells) to gain insights into the progression of neuroinflammation in sepsis.

In conclusion, we provide evidence that adenosine, a ubiquitous signaling molecule, behaves as an immune mediator of systemic inflammation to exacerbate neuroinflammation via astrocytic A1ARs, thereby driving the pathogenesis of SAE. Since A1ARs are the most abundant ARs expressed in the brain, understanding how A1ARs, which are expressed in other cell types (i.e., pericytes, microglia, oligodendrocyte precursor cells) as well, contribute to neuroinflammation will enhance our knowledge on adenosine signalling for inflammation-related CNS diseases and might be the basis for future therapeutical approaches.

Methods

Animals

This study involved the following animals maintained on C57BL/6 background: A1AR^fl/fl mice²⁸; Glast-CreERT2(CT2) mice⁶⁴, Cx3cr1-CreERT2 mice⁶⁵, NG2-CreERT2 mice⁶⁶; RiboTag mice (Rlp22HA)²⁹; GCaMP3 reporter mice (Rosa 26-CAG-lsl-GCAMP3)³⁰. To obtain cell type-specific A1AR knockout mice, A1AR^fl/fl mice were crossed to Glast-CreERT2 mice, Cx3cr1-CreERT2 mice, and NG2-CreERT2 mice to induce the specific knockout of A1ARs in astrocytes, microglia, and OPCs/pericytes, respectively, upon tamoxifen administration. For Fig. 1, Fig. 2b, c, and Supplementary Fig. 1, C57BL/6, A1AR^wt/wtxGlast^ct2/wt and A1AR^fl/flxGlast^wt/wt littermate mice were used as ‘wild-type’ (wt) control (ctl) mice without tamoxifen injection. For other experiments, A1AR^wt/wtxGlast^ct2/wt and A1AR^fl/flxGlast^wt/wt littermate mice were used as control (ctl) mice, also receiving tamoxifen injection.

RiboTag mice (Rlp22HA) were introduced to immunoprecipitate ribosome-associated translated mRNA in astrocytes upon breeding with A1AR^fl/flxGlast-CreERT2 mice. To visualize Ca²⁺ activity in astrocyte, GCaMP3 reporter mice were introduced to A1AR^fl/flxGlast-CreERT2 mice.

Mice of both sexes with 11–13 weeks age were used for most experiments (details in source data). All animals were maintained at the animal facility of the CIPMM under temperature- (22 °C ± 2 °C) and humidity- (45–65%) controlled conditions with 12 h light/dark cycle with an ad libitum supply of food and water. Animal husbandry and procedures were performed at the animal facility of CIPMM, University of Saarland according to European and German guidelines for the welfare of experimental animals. Animal experiments were approved by the Saarland state’s “Landesamt für Gesundheit und Verbraucherschutz” in Saarbrücken/Germany (animal license number: 65/2013, 12/2014, 34/2016, 36/2016, 03/2021 and 08/2021).

Tamoxifen (TAM), LPS treatment

As previously described⁶⁷, tamoxifen (CC99648, Carbolution) was dissolved in Miglyol (3274, Caesar & Loretz) at a concentration of 10 mg/ml and injected intraperitoneally to all mice crossed with CreERT2-driver mouse lines (100 mg/kg per body weight) for five consecutive days at the age of 4 weeks.

For the endotoxin challenge, 13 weeks old mice were injected intraperitoneally (i.p.) with 5 mg/kg of LPS (L2880, E. coli O55:B5, Sigma) or endotoxin-free PBS between 1 p.m. to 3 p.m. (CET) and kept for a maximum of 72 h post injection¹².

Anesthesia for the post-mortem animal experiments

All mice were anesthetized by i.p. injection of a low dose of ketamine/xylazin (120 and 12 mg/kg of body weight, respectively), followed by a lethal dose of ketamine/xylazin (240 and 24 mg/kg of body weight, respectively).

Plasma adenosine measurement

To measure plasma adenosine level, 0.4 ml blood was collected from the right ventricle of deeply anesthetized mice with a syringe containing 0.4 ml ice-cold stop solution (220 μM APCP (3633, Tocris), 100 μM NBMPR (N2255, Sigma), 40 μM dipyridamole (D9766, Sigma), 13.2 mM Na₂EDTA, 118 mM NaCl, 5 mM KCl), to block adenosine formation and transport. After centrifugation (1000 × g, 4 °C, 10 min), plasma was stored at −80 °C until analysis.

The plasma adenosine concentration was quantified with an adenosine assay kit (ab211094, Abcam) according to the protocol. The fluorescence was measured at excitation/emission = 535/587 nm.

Evaluation of blood brain barrier (BBB) permeability by Evans blue (EB)

For Fig. 1d EB (4% wt/vol in saline, 2 mL/kg) was administered through the tail vein 2 h before mice were euthanized. For Fig. 1c, mice were injected i.p. EB (4% wt/vol in saline, 10 mL/kg) 10 min prior to the i.p. injection of adenosine and were euthanized 2 h post the adenosine injection. Afterwards, Mice were perfused through the left ventricle with 10 ml ice-cold PBS to remove intravascular albumin-EB. Then half of the brains were quickly removed, weighed, and homogenized in 1 mL of PBS. After the first homogenization, 0.5 mL homogenization were mixed with 1.5 mL of 50% trichloroacetic acid, followed by vortex mixing for 2 min. After centrifugation (10,000 × g, 4 °C, 30 min), the supernatant was collected. 30 µl of supernatant was mixed with 90 µl 95% ethanol in a clear 96-well plate. The fluorescence intensity was measured at 620 nm excitation/680 nm emission on a microplate fluorescence reader and compared against a standard curve (serial dilutions of the stock dye solution in the concentration range of 0, 0.25, 0.5, 1, 5, 20 μg/mL). The Evans blue content was calculated and expressed as per gram of brain tissue.

Stereotactic adeno-associated viruses (AAV) injection

10-week-old mice were used for AAV injection as described before with some modifications³⁷. Briefly, mice were administered 0.1 mg/kg of buprenorphine (s.c.) subcutaneously and 0.2 mg/kg of dexamethasone (i.p.) before surgery. Subsequently, under continuous inhalational isoflurane anesthesia (5% for induction and 2% for maintenance with 66% O₂ and 33% N₂O), the mouse head was fitted and secured by blunt ear bars in a stereotactic apparatus (Robot stereotaxic, Neurostar) and the mouse eyes were covered by Bepanthen (Bayer, Leverkusen). After sterile cleaning and skin incision, viruses were injected at a rate of 0.1 μl min^–1 with a 10 µl Nanofil syringe (34 GA blunt needle, World Precision Instruments) into the striatum (1.1 mm anterior to bregma, ±1.2 mm from sagittal suture at a depth of 3 mm from the skull surface) or cortex (1.9 mm posterior to bregma, 1.5 mm from sagittal suture at a depth of 0.5 mm from the skull surface). The syringe was kept in place for 10 min after the injection was completed, to avoid liquid reflux. The skin was closed by simple interrupted sutures (non-absorbable, F.S.T.). Carprofen were administered once per day for three consecutive days and received tramadol hydrochloride in the drinking water (400 mg/L) after surgery. Mice were used for experiments 3 weeks post virus injection. Viruses used were: AAV2/5 GfaABC1D-GRAB_Ado virus (2.3 × 10¹² genome copies/ml); AAV2/5 GFAP-hM4Di-mCherry virus (3.04 × 10¹² genome copies/ml); AAV2/5 GFAP-tdTomato virus (1.1 × 10¹³ genome copies/ml), 0.8 μl for striatum, 0.5 μl for cortex, respectively.

Craniotomy and window implantation

The skull of the mice was exposed and underwent a craniotomy followed by removal of the dura^68,69 in correspondence of the primary somatosensory cortex (SSp-ctx; Ø 3-4 mm, centered 1.5-2 mm posterior to bregma, 1.5 mm from the sagittal medial axis). The glass coverslip (Ø 3 mm, No. 1.5, Glaswarenfabrik Karl Hecht GmbH) and a custom-made holder for head restraining were fixed with dental cement (RelyXTM Unicem 2 Clicker, 3 M Deutschland GmbH). Animals received canonical post-surgical care; three-day habituation training and imaging was performed one week after cranial window implantation.

In vivo imaging of extracellular adenosine level

In vivo imaging from GRAB_ado virus injected mice was performed using a custom-made two-photon laser-scanning microscope (2P-LSM) setup. Recordings started one week after cranial window implantation to enable animal recovery and habituation according to adapted protocols without water restriction^68,69. During image acquisition at different time points after an LPS challenge, awake mice were maintained head-fixed and placed into a smooth plastic tube to reduce vibration caused by the movement of the mice. In the drug administration experiments, the head-fixed mice received 1.5% isoflurane anesthesia delivered by means of a custom-made nose mask. Solutions of adenosine (0, 5, 10 or 20 mg/kg) and SR101 (20 mg/kg) were prepared in isotonic saline solution and administered after 200 frames of baseline recording (~88 s). Squared FOVs (512 ×512 μm) were chosen at a 60–80 μm depth from the surface and displaying a uniform virus expression with 910-nm laser. The laser power under the objective was adjusted from 5 to 30 mW, depending on the focal plane depth. Single focal plane images were acquired with a 2.28 Hz frame rate (1.4 µs pixel dwell time) and a resolution of 512 × 512 pixel.

Adenosine, adenosine analogue NECA, A1AR agonist CPA/CCPA, A1AR antagonist DPCPX treatment

To pharmacologically activate adenosine signaling, adenosine (5 mg/kg per body weight) (A9251, Sigma) was injected intraperitoneally every hour till 6 hours post first injection; NECA (1 mg/kg) (1691, Tocris) was injected intraperitoneally once at 0 hpi; CPA (1 mg/kg) (ab120398, abcam) was injected intraperitoneally once at 0 hpi; CCPA (0.3 mg/kg) (1705, Tocris) was injected intraperitoneally once at 0 hpi; DPCPX (1 mg/kg) (ab120396, Abcam) was injected intraperitoneally 4 hours after LPS (5 mg/kg) or Veh (1% DMSO in PBS) injection. To further amplify inflammatory response, CPA (1 mg/kg) was injected intraperitoneally 4 hours after LPS (1 mg/kg). Mice were analysed at 6 hours post injection.

Primary astrocyte culture and drug treatment

Astrocytes were cultured from ctl mice at postnatal day 0 (P0) to P1 as previously described⁷⁰. Briefly, hippocampi were dissected and treated with trypsin for 10 min at 37 °C. Tissues were dispersed through a cell strainer in culture medium (DMEM (Fisher Scientific) + 10% FCS (Fisher Scientific) + 0.1% Pen/Strep (Fisher Scientific) + 0.05% Mito Serum Extender (VWR) and centrifuged at 2300 rpm for 4 mins. Cells were plated into tissue culture flasks (ZHCL-Sarstedt) coated with collagen (1 mg/ml; Advanced BioMatrix) and kept in culture medium in a humidified 8.5% CO₂/91.5% air atmosphere at 37 °C. Confluent cultures (7–10 days) were shaken vigorously, the remaining astrocytes were trypsinized and plated in 6-well plates (ZHCL-Sarstedt). Purified astrocytes were used 5–7 d after plating until confluent. CCPA (30 nM) or CV1808 (50 nM) were added into the culture and incubated for 6 h. Subsequently, the cells were slightly rinsed with 1× PBS and homogenized in RLT buffer (Qiagen) for RNA extraction by RNeasy mini kit (74106, Qiagen).

Reverse transcription-polymerase chain reaction (RT-PCR)

Deeply anesthetized mice were perfused with ice-cold PBS. Cortex and striatum were dissected in ice cold PBS using an adult brain reference atlas. Total RNA of cortex and striatum were isolated with the RNeasy mini kit (74106, Qiagen) according to the instructions and underwent 15-min on-column DNase digestion using an RNase-Free DNase Set (79254, Qiagen). cDNA was prepared with reverse transcriptase using an Omniscript RT kit (205113, Qiagen) following the standard protocol provided. RT-PCR was performed using EvaGreen (27490, Axon) kit with CFX96 Real Time System (BioRad). The standard two step-program was used: 95 °C for 10 min, then 40 cycles at 95 °C for 15 sec, 60 °C for 1 min. The expressions of Gfap, Itgam, Pdgfra, Pdgfrb, Cxcl1, Cxcl10, Ccl2, Ccl5, Lcn2, Il6, Il1a, Il1b, Tnf were measured. β-actin was performed as a control in all qPCR analysis. Primers were designed to work at approximately + 60 °C and the specificity was assessed by melt curve analysis of each reaction indicating a single peak. Primer used in this study are listed in Supplementary Table 1. Relative expression of all targeted genes was determined using the ΔΔCt method with normalization to Actb expression.

Immunohistochemistry

Anesthetized mice were perfused with 1× PBS and 4% paraformaldehyde (PFA). Subsequently, the brain was dissected and post fixed in 4% PFA overnight (4 °C). Fixed brains were sliced into 35 μm thickness coronal sections in correspondence to the primary somatosensory cortex (AP −1.6 ± 0.5) and striatum (AP 0.5 ± 0.5), in PBS, using a Leica VT1000S vibratome and collected in 48-well culture plates containing 1× PBS. Vibratome sections were incubated for 1 h in blocking buffer (5% HS, 0.3% Triton X in 1× PBS) at room temperature. Sections were incubated with primary antibodies, diluted in the blocking solution overnight at 4 °C. The next day, sections were washed 3 times (10 min, 1× PBS) and incubated for 2 h with secondary antibodies and DAPI diluted in blocking buffer at room temperature in the dark. Subsequently, the sections were washed and mounted in Shandon ImmuMount (Thermo Scientific). For p-stat3 staining, slices in correspondence to the somatosensory cortex and striatum (AP −1.6 ± 0.5) was incubated in citrate buffer (pH = 6) at 95°C for 5 mins as antigen retrieval. Primary and secondary antibodies are listed in Supplementary Table 1: key resources.

Image acquisition and analysis

Whole brain slices were scanned with the automatic slide scanner AxioScan.Z1 (Zeiss, Oberkochen) as described before⁷¹. Cell counting from whole brain slices was manually performed using ZEN software (Zeiss, Jena). c-Fos intensity within Sox9⁺ and NeuN⁺ areas were automatically measured by using the machine learning function of the ZEN software. For the 3D reconstruction of microglia, confocal images were taken by LSM 710 and LSM880 confocal microscope (Zeiss, Oberkochen) with 1 μm intervals. Reconstruction of the microglial surface was performed using IMARIS (Version 9.6, Oxford Instruments) at the following settings: surface detail 0.700 μm (smooth); thresholding background subtraction (local contrast), diameter of largest sphere: 2.00. Next, the surface reconstruction was used as template for filament reconstruction with the following settings: detect new starting points: largest diameter 7.00 μm, seed points 0.300 μm; remove seed points around starting points: diameter of sphere regions: 15 μm. After filament reconstruction, individual data sets of Sholl analysis were exported into separate Excel files for further analysis. Image processing, three-dimensional reconstruction, and data analysis were performed in a blind manner regarding the experimental conditions.

Ribosome immunoprecipitation (IP)

After perfusion with ice-cold HBSS, cortical regions samples were dissected from mouse brain and stored at −80 °C until use. Tissues were homogenized in ice-cold lysis buffer (50 mM Tris, pH 7.4, 100 mM KCl, 12 mM MgCl₂, 1% NP-40, 1 mM DTT, 1× protease inhibitor, 200 units/ml RNasin (N2518, Promega) and 0.1 mg/ml cycloheximide (C7698, Sigma) in RNase-free deionized H₂O) 10% w/v with homogenizer (Precellys 24, PeQlab). Then homogenates were centrifuged at 10,000 × g at 4 °C for 10 min to remove cell debris. Supernatants were collected and removed: 50 μl were used as input analysis. Anti-HA Ab (1:100, MMS-101R, Covance) was added to the supernatant with slow rotation at 4 °C. Meanwhile, Dynabeads Protein G (10004D, Thermo Fisher Scientific) were equilibrated to the lysis buffer by washing three times. After 4 h of incubation with HA Ab, 100 μl pre-equilibrated beads were added to each sample and incubated overnight at 4 °C. After 10-12 h, Dynabeads were washed with high-salt buffer (50 mM Tris, 300 mM KCl, 12 mM MgCl₂, 1% NP-40, 1 mM DTT, 1× protease inhibitor, 100 units/ml RNasin and 0.1 mg/ml cycloheximide in RNase-free deionized H₂O) three times for 5 min at 4 °C. At the end of the washing, beads were magnetized and 350 µl RLT buffer from RNeasy Micro Kit (74004, Qiagen) was added to the beads. RNA was extracted followed with manufacturer’s instructions.

Next-generation RNA sequencing

The library was prepared and sequenced by Novogene using the following methods. Preliminary quality control was performed on 1% agarose gel electrophoresis to test RNA degradation and potential contamination. Sample purity and preliminary quantitation were measured using Bioanalyser 2100 (Agilent Technologies, USA), which was also used to check the RNA integrity and final quantitation. For library preparation, the mRNA present in the total RNA sample was isolated with magnetic beads of oligos d(T)25. This method is known as polyA-tailed mRNA enrichment. Subsequently, mRNA was randomly fragmented and cDNA synthesis proceeds using random hexamers and the reverse transcriptase enzyme. Once the synthesis of the first chain is finished, the second chain is synthesized with the addition of an Illumina buffer. Together with the presence of dNTPs, RNase H and polymerase I from E.coli, the second chain will be obtained by nick translation. The resulting products go through purification, end-repair, A-tailing and adapter ligation. Fragments of the appropriate size are enriched by PCR, where indexed P5 and P7 primers are introduced, and final products are purified. The library was checked with Qubit 2.0 and real-time PCR for quantification and bioanalyzer Agilent 2100 for size distribution detection. Quantified libraries were pooled and sequenced on Illumina Novaseq 6000 platform, according to effective library concentration and data amount.

The qualified libraries were sequenced next generation sequencing (NGS) based on Illumina’s sequencing technology by synthesis (SBS)- detection by fluorescence of the nucleotide added during the synthesis of the complementary chain—and in a parallelized and massive way. The Novaseq6000 sequencing system was used to sequence the libraries. The strategy is paired end 150 bp (PE150).

RNA-seq data processing

The RNA sequencing reads quality was assessed using FastQC (https://www.bioinformatics.babraham.ac.uk/projects/fastqc/). Reads were aligned to the GRCm38 Mus musculus genome using HISAT2 v2.0.5⁷² with default parameters. Gene count matrix of each sample was generated by featureCounts v1.5.0-p3⁷³. Downstream analysis was performed with the DEseq2 v1.20.0⁷⁴ package in R. Genes with normalized count below 10 were removed from downstream analysis. Significantly deregulated genes were identified by a false discovery rate lower than 0.05. Differential expression analysis between conditions was performed with the ‘DESeq’ function with default parameters. Log2 foldchange shrinkage was performed on the differential expression analysis result. Heatmaps of DEGs with p^adj value < 0.05 in any time point were visualized with pheatmap v1.0.12 using Z-scores. A K-means algorithm was used for unsupervised clustering of gene sets with similarities involved in different time points post LPS injection as used in previous studies^45,75. Selected gene set enrichment analysis of gene ontology (GO) and Kyoto Encyclopedia of Genes and Genomes (KEGG) pathway was performed with ClusterProfiler v3.8.1⁷⁶. Transcription factor prediction was performed using Metascape v3.5.20230501^77,78 with the differentially expressed genes identified by DEseq2.

Cytokine expression analysis

After perfusion with ice-cold PBS, the cortex and striatum were dissected from coronal brain slices (1 mm) and stored at −80 °C until further processing. For the cytokine array on brain homogenates, we used the Proteome Profiler Mouse Cytokine Array Kit (ARY006, R&D Systems) and Proteome Profiler Mouse XL Cytokine Array (ARY028, R&D Systems) following the manufacturer’s instructions. Briefly, brain tissue was homogenized in PBS containing 1× protease inhibitor cocktail (05892970001, Roche). Protein concentration was measured using the bicinchoninic acid (BCA) assay kit (23225, Thermo Fisher Scientific). 200 μg protein lysis were used for each membrane. Membranes were blocked, incubated, and washed according to standard protocol. Four membranes were exposed to X-ray film (47410, Fuji) for 15 minutes at the same time. The intensity (pixel density) of each spot-on membrane was quantified using Image J software (National Institutes of Health, Bethesda), corrected for background intensity, and normalized to control.

Flow cytometry analysis of immune cells

Flow cytometry analysis of infiltrated immune cells into the brain was performed and defined as previously described with some modifications⁷⁹. Adult mice brains were dissected after PBS/LPS injection and dissociated with the Adult Brain Dissociation Kit (Miltenyi Biotec, 130-107-677). The cell suspension was collected and washed with FACS buffer (1× PBS containing 3% fetal bovin serum). The preprared single cells were incubated with CD16/CD32 antibody (Miltenyi Biotec, 130-107-066) at 4 °C for 10 min to block Fc receptors. Afterwards, cells were stained with fluorophore-conjugated antibodies: CD3-APC-Cyanine7 (100221, BioLegend), CD11b-PerCP (101229, BioLegend), CD45-BV421 (103133, BioLegend), Ly6C-PE-Cyanine7 (128017, BioLegend) and Ly6G-APC (127613, BioLegend) at 4 °C for 30 min in the dark. After washing, cells were resuspended in FACS buffer for analysis by BD FACSVerse™ flow cytometer. The data were analyzed by Flowjo.

Acute brain slice preparation

Acute brain slice preparation was performed as previously described⁸⁰. Briefly, 11–13-week-old mice were anesthetized with isofluran (Abbvie, Ludwigshafen, Germany) and euthanized by cervical dislocation followed by decapitation. The brain was swiftly dissected and placed into ice-cooled, carbogen-saturated (5% CO₂, 95% O₂) cutting solution containing 87 mM NaCl, 3 mM KCl, 25 mM NaHCO₃, 1.25 mM NaH₂PO₄, 3 mM MgCl₂, 0.5 mM CaCl₂, 75 mM sucrose, and 25 mM glucose. 300 μm-thick sections in correspondence to the primary somatosensory cortex (SSp-ctx, AP −1.6 ± 0.6) were cut with a vibratome VT1200S (Leica Biosystems, Wetzlar, DE) using a 0.12 mm/s cutting speed and a 1.9 mm cutting amplitude. The procedure between decapitation and incubation was performed as fast as possible and in no longer than 10 min for optimal quality of the slice preparation. Slices were incubated for 30 min on a custom-made nylon-basket submersed in artificial cerebral spinal fluid (ACSF) containing 126 mM NaCl, 3 mM KCl, 25 mM NaHCO₃, 15 mM glucose, 1.2 mM NaH₂PO₄, 1 mM CaCl₂, and 2 mM MgCl₂ at 32 °C. Subsequently, brain slices were taken out of the water bath and placed to RT with continuous oxygenation before use.

Ca²⁺ imaging in hippocampal slices

For acute brain slices of 11–13-week-old GLAC^ct2/wtxA1AR^wt/wtxGCaMP3^fl/fl mice and GLAC^ct2/wtxA1AR^fl/flxGCaMP3^fl/fl mice were prepared as described above. Individual slices were transferred to a self-made imaging chamber under a custom-made 2P-LSM and fixed by stainless steel rings with 1 mm-spaced nylon fibres (Harp Slice Grid HSG-5A; ALA Scientific Instruments Inc., Farmingdale, NY, USA). A constant flow of oxygenated perfusion solution continuously perfused the imaging chamber at a flow rate of 2–5 ml/min by a peristaltic pump LKB P-1 (Pharmacia LKB, Uppsala, SE). Squared field of views (FOVs, 170 × 170 μm) from the cortical layers II-III of the SSp-ctx were chosen at a depth ranging from 30 to 100 μm from the slice surface and displaying a uniform astroglial distribution. Focal CPA (0.1 mg/ml) and SR101 (0.1 mg/ml) application was performed by means of borosilicate glass pipettes (BF150-86-10, Sutter Instrument, Novato, CA, US) mounted on 3-axis micromanipulator units (LN Mini 25, Luigs & Neumann GmbH, Ratingen, DE) controlled by a SM5 Remote Control station (Luigs & Neumann GmbH, Ratingen, DE). Pipettes were pulled using a micropipette Puller P-97 (Sutter Instrument, Novato, CA, US) to obtain a 5 μm-opening tip (0.5-1 MΩ). Cortical astrocytic Ca²⁺ activity was recorded upon drug application. Analysis of Ca²⁺ imaging data was performed using the custom-made detection and analysis software MATLAB (MSparkles v. 1.8.18)³² as previously described³¹. Shortly, fluorescence fluctuations at basal Ca²⁺ concentrations (F₀) were computed along the temporal axes of each individual pixel using a polynomial fitting in a least-squares sense. The range projection of ΔF/F0 was then used to identify local fluorescence maxima, serving as seed points for simultaneous, correlation-based growing of regions of activity (ROAs).

Electrophysiology of brain slices (LTP)

LTP recordings from dorsal hippocampus were performed as previously described^80,81. Briefly, acute hippocampal brain slices were prepared as mentioned above. Afterwards, slices were transferred to the recording chamber and continuously perfused with oxygenated ACSF containing (in mM)1 MgCl2 and 2.5 CaCl2 at a flow rate of 2–5 mL/min. Field excitatory postsynaptic potentials (fEPSP) were recorded by a micropipette of 1–3 MΩ resistance filled with ACSF in CA1 of hippocampus by stimulating Schaffer collaterals of CA3 using stimulus isolator and a biopolar electrode (WPI). Picrotoxin (50 μM) was perfused in the bath to inhibit ionotropic γ-aminobutyric acid type A receptors (GABAARs). Stimulus duration was 200 μs, current injection was 30–80 μA. To evoke LTP, triple θ-burst stimulation (TBS3) was used. TBS consisted of 10 bursts (4 pulses each burst, 100 Hz) delivered at an interburst interval of 200 ms, and repeated once at 10 s. The stimulation intensity was adjusted to evoke ∼30–60% of the maximum response. Waveform analysis was performed by Igor pro 6.3.7.2. The statistical analysis was conducted in Graphpad Prism. All experiments were conducted at RT.

Behavioral test

To evaluate the behavioural deficits following the LPS challenge, we evaluated open field test and sucrose preference test following the methods from previous studies with modifications^82,83. For the open field test, mice were placed at a random corner of the open field square (50 cm length × 50 cm width × 38 cm height) and positioned facing the wall. The movement of each mouse was recorded for 10 minutes. Open field test was performed before and after LPS challenge. Duration time in the center area (s), moved distance (cm) and speed (cm/s) were analyzed by EthoVision XT 11.5 (Noldus Technology). For the sucrose preference test, mice were single caged and habituated to the presence of two drinking bottles for 2 days. After the acclimatization, mice were presented to two drinking bottles: one containing 1% sucrose and the other tap water for 2 days in their cage. The positions of two drinking bottles were exchanged daily. Water and sucrose solution intake was measured daily by weighing the bottles. Sucrose preference was calculated as a percentage of the volume of sucrose intake over the total volume of fluid intake and averaged over the 2 days of testing. Sucrose preference test was performed before and after LPS challenge.

In vivo activation of hM4Di

CNO (half-life = ~0.5 h) was shown to activate hM4Di to enhance astrocytic Gi signaling for ~1.5−2 h in vivo⁸⁴. Therefore, three weeks after appropriate microinjection of AAV2/5-GFAP-hM4Di-mCherry or AAV2/5-GFAP-tdTomato into the striatum or cortex, CNO was administered two times to animals by intraperitoneal injection (2 mg/kg; dissolved in saline) at 2 hours and 4 hours post LPS challenge, respectively. 6 hours or 24 hours after LPS challenge, animals were used for behavior tests or immunohistochemistry.

Statistics and reproducibility

The statistical analyses of all data were performed with GraphPad Prism 9.5.1 statistical software (GraphPad, San Diego). For all immunostainings, two randomly selected brain slices of each mouse were studied. In addition, for the analysis of Iba1, more than 8 ROIs per mouse was analyzed. For normally distributed datasets, unpaired t tests, paired t tests (for studies of behavior), one-way ANOVA, and two-way ANOVA were used (indicated in each figure legend), while the Kruskal–Wallis test was used for non-normally distributed datasets. P values are indicated in the figures and legends. For the in vivo experiments, each data point represents the data obtained from a single mouse (except for electrophysiology). The total mouse numbers are indicated in the figure legends and source data. For electrophysiology, each data point refers to a slice and the mouse number is indicated in the figure legends. Normal distributed datasets are shown as mean ± SEM. else are shown as the median ± IQR are indicated as thick and thin dashed lines, respectively. p value of ≤0.05 was considered statistically significant.

Reporting summary

Further information on research design is available in the Nature Portfolio Reporting Summary linked to this article.

Data availability

The data supporting the findings of this study are available from the corresponding authors upon request. The RNA sequencing data have been deposited in the GEO database GSE248275. Source data are provided with this paper.

Code availability

Custom-written R codes have been made available on Github [https://github.com/qilinguo1005/Adenosine-triggers-early-astrocyte-reactivity.git].

Change history

18 September 2024
A Correction to this paper has been published: https://doi.org/10.1038/s41467-024-52497-x

References

van der Poll, T., van de Veerdonk, F. L., Scicluna, B. P. & Netea, M. G. The immunopathology of sepsis and potential therapeutic targets. Nat. Rev. Immunol. 17, 407–420 (2017).
Article PubMed Google Scholar
Mazeraud, A. et al. Septic-associated encephalopathy: a comprehensive review. Neurotherapeutics 17, 392–403 (2020).
Article PubMed PubMed Central Google Scholar
Dantzer, R., O’Connor, J. C., Freund, G. G., Johnson, R. W. & Kelley, K. W. From inflammation to sickness and depression: when the immune system subjugates the brain. Nat. Rev. Neurosci. 9, 46–56 (2008).
Article CAS PubMed PubMed Central Google Scholar
Manabe, T. & Heneka, M. T. Cerebral dysfunctions caused by sepsis during ageing. Nat. Rev. Immunol. 22, 444–458 (2022).
Article CAS PubMed Google Scholar
Duan, L. et al. PDGFRβ cells rapidly relay inflammatory signal from the circulatory system to neurons via chemokine CCL2. Neuron 100, 183–200.e188 (2018).
Article CAS PubMed Google Scholar
Kodali, M. C., Chen, H. & Liao, F. F. Temporal unsnarling of brain’s acute neuroinflammatory transcriptional profiles reveals panendothelitis as the earliest event preceding microgliosis. Mol. Psychiatry 26, 3905–3919 (2021).
Article CAS PubMed Google Scholar
Fritz, M. et al. Prostaglandin-dependent modulation of dopaminergic neurotransmission elicits inflammation-induced aversion in mice. J. Clin. Invest. 126, 695–705 (2016).
Article PubMed Google Scholar
Martin, C., Leone, M., Viviand, X., Ayem, M. L. & Guieu, R. High adenosine plasma concentration as a prognostic index for outcome in patients with septic shock. Crit. Care Med. 28, 3198–3202 (2000).
Article CAS PubMed Google Scholar
Sumi, Y. et al. Plasma ATP is required for neutrophil activation in a mouse sepsis model. Shock 42, 142–147 (2014).
Article CAS PubMed PubMed Central Google Scholar
Ramakers, B. P. et al. Circulating adenosine increases during human experimental endotoxemia but blockade of its receptor does not influence the immune response and subsequent organ injury. Crit. Care 15, R3 (2011).
Article PubMed PubMed Central Google Scholar
Wu, Z. et al. A sensitive GRAB sensor for detecting extracellular ATP in vitro and in vivo. Neuron 110, 770–782.e775 (2022).
Article CAS PubMed Google Scholar
Hasel, P., Rose, I. V. L., Sadick, J. S., Kim, R. D. & Liddelow, S. A. Neuroinflammatory astrocyte subtypes in the mouse brain. Nat. Neurosci. 24, 1475–1487 (2021).
Article CAS PubMed Google Scholar
Liddelow, S. A. et al. Neurotoxic reactive astrocytes are induced by activated microglia. Nature 541, 481–487 (2017).
Article ADS CAS PubMed PubMed Central Google Scholar
Kang, S. S. et al. Lipocalin-2 protects the brain during inflammatory conditions. Mol. Psychiatry 23, 344–350 (2018).
Article CAS PubMed Google Scholar
Borea, P. A., Gessi, S., Merighi, S., Vincenzi, F. & Varani, K. Pathological overproduction: the bad side of adenosine. Br. J. Pharm. 174, 1945–1960 (2017).
Article CAS Google Scholar
Borea, P. A., Gessi, S., Merighi, S. & Varani, K. Adenosine as a multi-signalling guardian angel in human diseases: when, where and how does it exert its protective effects. Trends Pharm. Sci. 37, 419–434 (2016).
Article CAS PubMed Google Scholar
Meng, F. et al. CD73-derived adenosine controls inflammation and neurodegeneration by modulating dopamine signalling. Brain 142, 700–718 (2019).
Article PubMed Google Scholar
Haruwaka, K. et al. Dual microglia effects on blood brain barrier permeability induced by systemic inflammation. Nat. Commun. 10, 5816 (2019).
Article ADS CAS PubMed PubMed Central Google Scholar
Carman, A. J., Mills, J. H., Krenz, A., Kim, D. G. & Bynoe, M. S. Adenosine receptor signaling modulates permeability of the blood-brain barrier. J. Neurosci. 31, 13272–13280 (2011).
Article CAS PubMed PubMed Central Google Scholar
Peng, W. et al. Regulation of sleep homeostasis mediator adenosine by basal forebrain glutamatergic neurons. Science 369, https://doi.org/10.1126/science.abb0556 (2020).
Gourine, A. V. et al. Release of ATP in the central nervous system during systemic inflammation: real-time measurement in the hypothalamus of conscious rabbits. J. Physiol. 585, 305–316 (2007).
Article CAS PubMed PubMed Central Google Scholar
Chiu, G. S. et al. Adenosine through the A2A adenosine receptor increases IL-1β in the brain contributing to anxiety. Brain Behav. Immun. 41, 218–231 (2014).
Article CAS PubMed PubMed Central Google Scholar
Agnew-Svoboda, W. et al. A genetic tool for the longitudinal study of a subset of post-inflammatory reactive astrocytes. Cell Rep. Methods 2, 100276 (2022).
Article CAS PubMed PubMed Central Google Scholar
Bynoe, M. S., Viret, C., Yan, A. & Kim, D. G. Adenosine receptor signaling: a key to opening the blood-brain door. Fluids Barriers CNS 12, 20 (2015).
Article PubMed PubMed Central Google Scholar
Zhang, Y. et al. An RNA-sequencing transcriptome and splicing database of glia, neurons, and vascular cells of the cerebral cortex. J. Neurosci. 34, 11929–11947 (2014).
Article CAS PubMed PubMed Central Google Scholar
Ximerakis, M. et al. Single-cell transcriptomic profiling of the aging mouse brain. Nat. Neurosci. 22, 1696–1708 (2019).
Article CAS PubMed Google Scholar
Motori, E. et al. Inflammation-induced alteration of astrocyte mitochondrial dynamics requires autophagy for mitochondrial network maintenance. Cell Metab. 18, 844–859 (2013).
Article CAS PubMed Google Scholar
Scammell, T. E. et al. Focal deletion of the adenosine A1 receptor in adult mice using an adeno-associated viral vector. J. Neurosci. 23, 5762–5770 (2003).
Article CAS PubMed PubMed Central Google Scholar
Sanz, E. et al. Cell-type-specific isolation of ribosome-associated mRNA from complex tissues. Proc. Natl. Acad. Sci. USA 106, 13939–13944 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Paukert, M. et al. Norepinephrine controls astroglial responsiveness to local circuit activity. Neuron 82, 1263–1270 (2014).
Article CAS PubMed PubMed Central Google Scholar
Rieder, P. et al. Astrocytes and microglia exhibit cell-specific Ca. Front. Mol. Neurosci. 15, 840948 (2022).
Article CAS PubMed PubMed Central Google Scholar
Stopper, G. et al. Novel algorithms for improved detection and analysis of fluorescent signal fluctuations. Pflug. Arch. https://doi.org/10.1007/s00424-023-02855-3 (2023).
Article Google Scholar
Nagai, J. et al. Hyperactivity with disrupted attention by activation of an astrocyte synaptogenic cue. Cell 177, 1280–1292.e1220 (2019).
Article CAS PubMed PubMed Central Google Scholar
He, Q., Wang, J. & Hu, H. Illuminating the activated brain: emerging activity-dependent tools to capture and control functional neural circuits. Neurosci. Bull. 35, 369–377 (2019).
Article CAS PubMed Google Scholar
Jonnalagadda, D. et al. FTY720 requires vitamin B(12)-TCN2-CD320 signaling in astrocytes to reduce disease in an animal model of multiple sclerosis. Cell Rep. 42, 113545 (2023).
Article CAS PubMed PubMed Central Google Scholar
Hernandez, V. G. et al. Translatome analysis reveals microglia and astrocytes to be distinct regulators of inflammation in the hyperacute and acute phases after stroke. Glia 71, 1960–1984 (2023).
Article CAS PubMed PubMed Central Google Scholar
Nagai, J. et al. Specific and behaviorally consequential astrocyte Gq GPCR signaling attenuation in vivo with iβARK. Neuron 109, 2256–2274.e2259 (2021).
Article CAS PubMed PubMed Central Google Scholar
Giovannoni, F. & Quintana, F. J. The role of astrocytes in CNS inflammation. Trends Immunol. 41, 805–819 (2020).
Article CAS PubMed PubMed Central Google Scholar
Han, R. T., Kim, R. D., Molofsky, A. V. & Liddelow, S. A. Astrocyte-immune cell interactions in physiology and pathology. Immunity 54, 211–224 (2021).
Article CAS PubMed Google Scholar
Sofroniew, M. V. Astrocyte reactivity: subtypes, states, and functions in CNS innate immunity. Trends Immunol. 41, 758–770 (2020).
Article CAS PubMed PubMed Central Google Scholar
Borst, K., Dumas, A. A. & Prinz, M. Microglia: Immune and non-immune functions. Immunity 54, 2194–2208 (2021).
Article CAS PubMed Google Scholar
Linnerbauer, M., Wheeler, M. A. & Quintana, F. J. Astrocyte crosstalk in CNS inflammation. Neuron 108, 608–622 (2020).
Article CAS PubMed PubMed Central Google Scholar
Huang, X. et al. Microglial IL-1RA ameliorates brain injury after ischemic stroke by inhibiting astrocytic CXCL1-mediated neutrophil recruitment and microvessel occlusion. Glia 71, 1607–1625 (2023).
Article CAS PubMed Google Scholar
Rummel, C., Inoue, W., Poole, S. & Luheshi, G. N. Leptin regulates leukocyte recruitment into the brain following systemic LPS-induced inflammation. Mol. Psychiatry 15, 523–534 (2010).
Article CAS PubMed Google Scholar
Shemer, A. et al. Interleukin-10 prevents pathological microglia hyperactivation following peripheral endotoxin challenge. Immunity 53, 1033–1049.e1037 (2020).
Article CAS PubMed Google Scholar
Wu, K. C., Lee, C. Y., Chern, Y. & Lin, C. J. Amelioration of lipopolysaccharide-induced memory impairment in equilibrative nucleoside transporter-2 knockout mice is accompanied by the changes in glutamatergic pathways. Brain Behav. Immun. 96, 187–199 (2021).
Article CAS PubMed Google Scholar
Izumi, Y. et al. A proinflammatory stimulus disrupts hippocampal plasticity and learning via microglial activation and 25-hydroxycholesterol. J. Neurosci. 41, 10054–10064 (2021).
Article CAS PubMed PubMed Central Google Scholar
Klawonn, A. M. et al. Microglial activation elicits a negative affective state through prostaglandin-mediated modulation of striatal neurons. Immunity 54, 225–234.e226 (2021).
Article CAS PubMed Google Scholar
Welsh, T. G. & Kucenas, S. Purinergic signaling in oligodendrocyte development and function. J. Neurochem. 145, 6–18 (2018).
Article CAS PubMed PubMed Central Google Scholar
Boison, D. Adenosine as a neuromodulator in neurological diseases. Curr. Opin. Pharmacol. 8, 2–7 (2008).
Article CAS PubMed Google Scholar
Benarroch, E. Adenosine and its receptors - multiple modulatory functions and potential therapeutic targets for neurologic disease. Neurology 70, 231–236 (2008).
Article PubMed Google Scholar
Chiu, G. & Freund, G. Modulation of neuroimmunity by adenosine and its receptors: metabolism to mental illness. Metab. Clin. Exp. 63, 1491–1498 (2014).
Article CAS PubMed Google Scholar
Latini, S. & Pedata, F. Adenosine in the central nervous system: release mechanisms and extracellular concentrations. J. Neurochem. 79, 463–484 (2001).
Article CAS PubMed Google Scholar
Mikitsh, J. L. & Chacko, A. M. Pathways for small molecule delivery to the central nervous system across the blood-brain barrier. Perspect. Med. Chem. 6, 11–24 (2014).
Google Scholar
Mills, J. H. et al. CD73 is required for efficient entry of lymphocytes into the central nervous system during experimental autoimmune encephalomyelitis. Proc. Natl Acad. Sci. USA 105, 9325–9330 (2008).
Article ADS CAS PubMed PubMed Central Google Scholar
Zhao, Z. et al. Bacteria elevate extracellular adenosine to exploit host signaling for blood-brain barrier disruption. Virulence 11, 980–994 (2020).
Article CAS PubMed PubMed Central Google Scholar
Ramakers, B. P., Riksen, N. P., van der Hoeven, J. G., Smits, P. & Pickkers, P. Modulation of innate immunity by adenosine receptor stimulation. Shock 36, 208–215 (2011).
Article CAS PubMed Google Scholar
Patani, R., Hardingham, G. E. & Liddelow, S. A. Functional roles of reactive astrocytes in neuroinflammation and neurodegeneration. Nat. Rev. Neurol. 19, 395–409 (2023).
Article CAS PubMed Google Scholar
Novakovic, M. M. et al. Astrocyte reactivity and inflammation-induced depression-like behaviors are regulated by Orai1 calcium channels. Nat. Commun. 14, 5500 (2023).
Article ADS CAS PubMed PubMed Central Google Scholar
Shigetomi, E., Saito, K., Sano, F. & Koizumi, S. Aberrant calcium signals in reactive astrocytes: a key process in neurological disorders. Int. J. Mol. Sci. 20, https://doi.org/10.3390/ijms20040996 (2019).
Ceyzériat, K. & Abjean, L. Carrillo-de Sauvage, M. A., Ben Haim, L. & Escartin, C. The complex STATes of astrocyte reactivity: How are they controlled by the JAK-STAT3 pathway? Neuroscience 330, 205–218 (2016).
Article PubMed Google Scholar
White, C. D. & Sacks, D. B. Regulation of MAP kinase signaling by calcium. Methods Mol. Biol. 661, 151–165 (2010).
Article CAS PubMed Google Scholar
Hösli, L. et al. Direct vascular contact is a hallmark of cerebral astrocytes. Cell Rep. 39, 110599 (2022).
Article PubMed Google Scholar
Mori, T. et al. Inducible gene deletion in astroglia and radial glia - a valuable tool for functional and lineage analysis. Glia 54, 21–34 (2006).
Article PubMed Google Scholar
Jung, S. et al. Analysis of fractalkine receptor CX(3)CR1 function by targeted deletion and green fluorescent protein reporter gene insertion. Mol. Cell Biol. 20, 4106–4114 (2000).
Article CAS PubMed PubMed Central Google Scholar
Huang, W. et al. Novel NG2-CreERT2 knock-in mice demonstrate heterogeneous differentiation potential of NG2. Glia 62, 896–913 (2014).
Article PubMed Google Scholar
Liu, Q. et al. Specific detection and deletion of the sigma-1 receptor widely expressed in neurons and glial cells in vivo. J. Neurochem. 164, 764–785 (2023).
Article CAS PubMed Google Scholar
Cupido, A., Catalin, B., Steffens, H. & Kirchhoff, F. Surgical procedures to study microglial motility in the brain and in the spinal cord by in vivo two-photon laser-scanning microscopy. In: Laser scanning microscopy and quantitative image analysis of neuronal tissue, 37–50 (2014).
Kislin, M. et al. Flat-floored air-lifted platform: a new method for combining behavior with microscopy or electrophysiology on awake freely moving rodents. JoVE 88, e51869 (2014).
Knapp, M. L. et al. A longer isoform of Stim1 is a negative SOCE regulator but increases cAMP-modulated NFAT signaling. EMBO Rep. 23, e53135 (2022).
Article CAS PubMed Google Scholar
Huang, W., Bai, X., Meyer, E. & Scheller, A. Acute brain injuries trigger microglia as an additional source of the proteoglycan NG2. Acta Neuropathol. Commun. 8, 146 (2020).
Article CAS PubMed PubMed Central Google Scholar
Kim, D., Paggi, J. M., Park, C., Bennett, C. & Salzberg, S. L. Graph-based genome alignment and genotyping with HISAT2 and HISAT-genotype. Nat. Biotechnol. 37, 907 (2019).
Article CAS PubMed PubMed Central Google Scholar
Liao, Y., Smyth, G. K. & Shi, W. featureCounts: an efficient general purpose program for assigning sequence reads to genomic features. Bioinformatics 30, 923–930 (2014).
Article CAS PubMed Google Scholar
Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).
Do, J. H. & Choi, D. K. Clustering approaches to identifying gene expression patterns from DNA microarray data. Mol. Cells 25, 279–288 (2008).
Article CAS PubMed Google Scholar
Yu, G., Wang, L.-G., Han, Y. & He, Q.-Y. clusterProfiler: an R package for comparing biological themes among gene clusters. Omics 16, 284–287 (2012).
Article CAS PubMed PubMed Central Google Scholar
Zhou, Y. et al. Metascape provides a biologist-oriented resource for the analysis of systems-level datasets. Nat. Commun. 10, 1523 (2019).
Article ADS PubMed PubMed Central Google Scholar
Han, H. et al. TRRUST v2: an expanded reference database of human and mouse transcriptional regulatory interactions. Nucleic Acids Res. 46, D380–d386 (2018).
Article CAS PubMed Google Scholar
Cazareth, J., Guyon, A., Heurteaux, C., Chabry, J. & Petit-Paitel, A. Molecular and cellular neuroinflammatory status of mouse brain after systemic lipopolysaccharide challenge: importance of CCR2/CCL2 signaling. J. Neuroinflamm. 11, 1–15 (2014).
Article Google Scholar
Zhao, N., Huang, W., Cãtãlin, B., Scheller, A. & Kirchhoff, F. L-Type Ca2+ channels of NG2 glia determine proliferation and NMDA receptor-dependent plasticity. Front. Cell Dev. Biol. 9, 759477 (2021).
Article PubMed PubMed Central Google Scholar
Wang, H. et al. Metabotropic glutamate receptors induce a form of LTP controlled by translation and Arc signaling in the hippocampus. J. Neurosci. 36, 1723–1729 (2016).
Article CAS PubMed PubMed Central Google Scholar
Liu, M. Y. et al. Sucrose preference test for measurement of stress-induced anhedonia in mice. Nat. Protoc. 13, 1686–1698 (2018).
Article CAS PubMed Google Scholar
Fang, L.-P. et al. Impaired bidirectional communication between interneurons and oligodendrocyte precursor cells affects social cognitive behavior. Nat. Commun. 13, 1394 (2022).
Article ADS CAS PubMed PubMed Central Google Scholar
Vaidyanathan, T. V., Collard, M., Yokoyama, S., Reitman, M. E. & Poskanzer, K. E. Cortical astrocytes independently regulate sleep depth and duration via separate GPCR pathways. Elife 10, e63329 (2021).
Article CAS PubMed PubMed Central Google Scholar

Download references

Acknowledgements

We thank Daniel Schauenburg and colleagues for excellent animal husbandry. We thank Dr. Yulong Li (Peking University) for providing the AAV-GRAB_Ado1.0 plasmids; Dr. Amit Agarwal (University of Heidelberg) for providing Rosa26-GCaMP3 mice, Dr. André Zeug (Hannover Medical School) for providing the AAV2/5-GFAP-tdTomato virus. This work was supported by grants from the Deutsche Forschungsgemeinschaft (HU 2614/1-1 (Project No. 462650276) to W.H., Sino-German joint project KI 503/14-1 to W.H. and F.K., SPP 1757, SFB 894, SFB 1158 to F.K.); the Fritz Thyssen Foundation (10.21.1.021MN) and the Medical faculty of the University of Saarland (HOMFOR2016, HOMFORexzellent2017, HOMFOR2024 Anschubfinanzierung) to W.H.; the BMBF (EraNet-Neuron BrIE) and the European Commission (EC-H2020 FET ProAct Neurofibres) to F.K. The flow cytometry platform is funded by INST 256/423-1 FUGG from DFG. The collaborative work of W.H., F.K., and S.B. was supported by the Mobility Project (M-0679) from the Sino-German Research Center for Research Promotion. Q.L. was supported by a PhD student fellowship of the Chinese Scholarship Council.

Funding

Open Access funding enabled and organized by Projekt DEAL.

Author information

Authors and Affiliations

Molecular Physiology, Center for Integrative Physiology and Molecular Medicine (CIPMM), University of Saarland, 66421, Homburg, Germany
Qilin Guo, Davide Gobbo, Na Zhao, Qing Liu, Li-Pao Fang, Xianshu Bai, Anja Scheller, Frank Kirchhoff & Wenhui Huang
Center for Gender-specific Biology and Medicine (CGBM), University of Saarland, 66421, Homburg, Germany
Qilin Guo, Li-Pao Fang, Xianshu Bai, Anja Scheller, Frank Kirchhoff & Wenhui Huang
Institute of Anatomy and Cell Biology, University of Saarland, 66421, Homburg, Germany
Na Zhao
Biophysics, CIPMM, University of Saarland, 66421, Homburg, Germany
Hong Zhang & Renping Zhao
Molecular Neurophysiology, CIPMM, University of Saarland, 66421, Homburg, Germany
Nana-Oye Awuku
Department of Experimental and Clinical Toxicology, Institute of Experimental and Clinical Pharmacology and Toxicology, Center for Molecular Signaling (PZMS), University of Saarland, 66421, Homburg, Germany
Tanja M. Gampfer & Markus R. Meyer
Institute for Regenerative Medicine, Shanghai East Hospital, Frontier Science Center for Stem Cell Research, School of Life Sciences and Technology, Tongji University, 200092, Shanghai, China
Shan Bian

Authors

Qilin Guo
View author publications
You can also search for this author in PubMed Google Scholar
Davide Gobbo
View author publications
You can also search for this author in PubMed Google Scholar
Na Zhao
View author publications
You can also search for this author in PubMed Google Scholar
Hong Zhang
View author publications
You can also search for this author in PubMed Google Scholar
Nana-Oye Awuku
View author publications
You can also search for this author in PubMed Google Scholar
Qing Liu
View author publications
You can also search for this author in PubMed Google Scholar
Li-Pao Fang
View author publications
You can also search for this author in PubMed Google Scholar
Tanja M. Gampfer
View author publications
You can also search for this author in PubMed Google Scholar
Markus R. Meyer
View author publications
You can also search for this author in PubMed Google Scholar
Renping Zhao
View author publications
You can also search for this author in PubMed Google Scholar
Xianshu Bai
View author publications
You can also search for this author in PubMed Google Scholar
Shan Bian
View author publications
You can also search for this author in PubMed Google Scholar
Anja Scheller
View author publications
You can also search for this author in PubMed Google Scholar
Frank Kirchhoff
View author publications
You can also search for this author in PubMed Google Scholar
Wenhui Huang
View author publications
You can also search for this author in PubMed Google Scholar

Contributions

W.H. conceptualized the project and designed experiments with input from F.K. and Q.G. W.H. and F.K. supervised the study and ensured the coordination and resource support of the project. Q.G. performed RiboTag immunoprecipitation, immunohistochemistry, immunoblot, qPCR, confocal imaging and analysis, RNA-seq analysis, and behavioral tests. Q.G. and D.G. performed an AAV injection. Q.G., D.G., and W.H. carried out in vivo 2P-LSM imaging. D.G. performed ex vivo slice imaging and all 2P-LSM imaging analysis. N.Z. performed LTP recordings. Q.G., T.G., and M.R.M. performed plasma adenosine concentration measurements. Q.L. contributed to immunohistochemistry and behavioral tests. L-P.F., X.B., and S.B. contributed to sample collection and qPCR. H.Z. and R.Z. performed flow cytometry, and N-O.K. carried out the primary astrocyte cultures. A.S. performed AxioScan imaging. Q.G. analyzed data and generated figures. W.H. and Q.G. wrote the manuscript with input from all the other authors. F.K. revised the manuscript.

Corresponding authors

Correspondence to Frank Kirchhoff or Wenhui Huang.

Ethics declarations

Competing interests

The authors declare no competing interests

Peer review

Peer review information

Nature Communications thanks Veit Rothhammer, Jun Nagai and the other anonymous reviewer(s) for their contribution to the peer review of this work. A peer review file is available.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Supplementary Information

Reporting Summary

Peer Review File

Description of Additional Supplementary Files

Supplementary Video 1

Supplementary Video 2

Source data

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/.

Reprints and permissions

About this article

Cite this article

Guo, Q., Gobbo, D., Zhao, N. et al. Adenosine triggers early astrocyte reactivity that provokes microglial responses and drives the pathogenesis of sepsis-associated encephalopathy in mice. Nat Commun 15, 6340 (2024). https://doi.org/10.1038/s41467-024-50466-y

Download citation

Received: 10 November 2023
Accepted: 11 July 2024
Published: 27 July 2024
DOI: https://doi.org/10.1038/s41467-024-50466-y

This article is cited by

Astrocytic adenosine A1 receptors: a new potential target for treating sepsis-associated encephalopathy
- Si-Le Liu
- Yong Tang
Purinergic Signalling (2024)

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.