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Fractalkine (CX3CL1) enhances hippocampal N-methyl-d-aspartate receptor (NMDAR) function via d-serine and adenosine receptor type A2 (A2AR) activity
Journal of Neuroinflammationvolume 10, Article number: 876 (2013)
N-Methyl-d-aspartate receptors (NMDARs) play fundamental roles in basic brain functions such as excitatory neurotransmission and learning and memory processes. Their function is largely regulated by factors released by glial cells, including the coagonist d-serine. We investigated whether the activation of microglial CX3CR1 induces the release of factors that modulate NMDAR functions.
We recorded the NMDAR component of the field excitatory postsynaptic potentials (NMDA-fEPSPs) elicited in the CA1 stratum radiatum of mouse hippocampal slices by Shaffer collateral stimulation and evaluated d-serine content in the extracellular medium of glial primary cultures by mass spectrometry analysis.
We demonstrated that CX3CL1 increases NMDA-fEPSPs by a mechanism involving the activity of the adenosine receptor type A2 (A2AR) and the release of the NMDAR coagonist d-serine. Specifically (1) the selective A2AR blocker 7-(2-phenylethyl)-5-amino-2-(2-furyl)-pyrazolo-[4,3-e]-1,2,4-triazolo[1,5-c]pyrimidine (SCH58261) and the genetic ablation of A2AR prevent CX3CL1 action while the A2AR agonist 5-(6-amino-2-(phenethylthio)-9H-purin-9-yl)-N-ethyl-3,4-dihydroxytetrahydrofuran-2-carboxamide (VT7) mimics CX3CL1 effect, and (2) the selective blocking of the NMDAR glycine (and d-serine) site by 5,7-dicholorokynurenic acid (DCKA), the enzymatic degradation of d-serine by d-amino acid oxidase (DAAO) and the saturation of the coagonist site by d-serine, all block the CX3CL1 effect. In addition, mass spectrometry analysis demonstrates that stimulation of microglia and astrocytes with CX3CL1 or VT7 increases d-serine release in the extracellular medium.
CX3CL1 transiently potentiates NMDAR function though mechanisms involving A2AR activity and the release of d-serine.
It is now widely accepted that, in addition to their well established role in the immune system, chemokines and their receptors play important roles in the central nervous system (CNS), contributing to the homeostasis of mature brain through neuroendocrine modulation, neuromodulation and neuroglia communication (for review see  and ).
Fractalkine (CX3CL1) is one of the chemokines most abundantly expressed in the brain [3–5], especially by neurons, whereas the only known CX3CL1 receptor, CX3CR1, is expressed by microglial cells [5–7]. The CX3CR1/CX3CL1 axis plays a major role in neuron/microglia crosstalk and in neuroprotection under conditions of inflammation/injury [5, 8–10]. We have previously shown that CX3CL1 reduces neuronal death induced by glutamate (Glu)  through microglia-derived protective factors including adenosine [12, 13] and in rodent models of permanent ischemia, exogenous CX3CL1 administration is neuroprotective . Moreover, at synapses between Schaffer collaterals and pyramidal neurons in the CA1 region of the hippocampus, CX3CL1 exerts a neuromodulatory role inducing α-amino-3-hydroxy-5-methyl-4-isoxazolepropionic acid receptor (AMPAR)-mediated excitatory synaptic depression and negatively modulating long-term potentiation (LTP) mediated by N-methyl-d-aspartate receptors (NMDAR) [15–17].
It is well established that NMDARs play an important role in a variety of physiological and pathological processes such as excitatory neurotransmission, synaptic plasticity and excitotoxicity [18, 19]. NMDAR function is regulated by agents acting on a number of sites other than the Glu binding site , such as glycine  and d-serine that act with different affinities on the same binding site . A recent report describes that d-serine preferentially acts on synaptic NMDARs, whereas glycine acts on extrasynaptic NMDARs . In addition, d-serine is highly localized on glia in areas of the brain particularly enriched in NMDARs , thus suggesting that these cells are likely playing key roles in regulating NMDAR-dependent processes including synaptic transmission and synaptic plasticity. d-serine is degraded by d-amino acid oxidase (DAAO) and is mainly synthesized from l-serine by serine racemase (SR) present primarily on astrocytes. Recent studies also identified neurons and microglia as other important cellular sources of serine in the brain [25–29] even thought the role of neuronal and microglial d-serine remains to be determined.
Microglia have long been characterized by their innate immune activity in the nervous system, however recent evidence has shed new light on microglia function. These cells are now recognized as full time partners in neuronal function and the crosstalk between neurons and microglia has been described in several physiological and pathological conditions. Microglia secrete a number of factors, including Glu, nitric oxide, purines, trophic and anti-inflammatory substances , but also soluble factors affecting NMDAR and AMPAR such as glycine, cytokines, serine proteases and adenosine [31–34]. We have previously shown that stimulation of microglial cells with CX3CL1 induces the release of adenosine, which mediates the reduction of AMPAR function [13, 15–17], but scarce information is available on specific CX3CL1 effects on hippocampal NMDARs  that are highly involved in synaptic plasticity processes.
In the present work we demonstrate that CX3CL1 modulates NMDA-mediated synaptic transmission in the hippocampal CA1 region, through the activity of the A2AR and the release of d-serine from glia.
Experiments were performed in agreement with international guidelines on the ethical use of animals from the European Communities Council Directive of 24 November 1986 (86/609 EEC). Hippocampal slices were routinely obtained from 1-month-old C57BL/6. When specified, hippocampal slices were obtained from gene modified animals: (1) CX3CR1GFP/GFP mice on the C57BL/6 background (from Charles River, Calco, Italy), that were generated by replacing the first 390 bp of the CX 3 CR1 gene with the EGFP gene [6, 36]; (2) A1R KO mice  and (3) A3RKO mice  backcrossed at least ten times on a C57BL/6 background; (4) A2 knockout mice  on a BALB/cJ background (C;129S-Adora2a tm1Jfc/J) and control BALB/cJ wild-type mice (Charles River, Calco, Italy). C57BL/6 and BALB/cJ wild-type mice showed similar responses to CX3CL1 application (not shown).
Hippocampal slice preparation
Briefly, animals were decapitated after being anesthetized with halothane. Whole brains were rapidly removed from the skull and immersed for 10 minutes in ice-cold artificial cerebrospinal fluid (ACSF) solution containing (1) for field recording experiments (in mM): NaCl 125, KCl 4.4, CaCl2 2.5, MgSO4 1.5, NaHPO4 1, NaHCO3 26 and glucose 10; (2) for patch clamp recordings (in mM): NaCl 125, KCl 2.5, NaH2PO4 1.25, NaHCO3 26, CaCl2 2, MgCl2 1, and glucose 10. The ACSF was continuously oxygenated with 95% O2, 5% CO2 to maintain the proper pH (7.4). Transverse (250 or 350 μm thick) slices were cut at 4°C with a vibratome (DSK, Japan) and the slices were placed in a chamber containing oxygenated ACSF. After their preparation, slices were allowed to recover for 1 h before recording.
For field recording experiments individual slices (350 μm thick) were then transferred to the interface slice-recording chamber (BSC1, Scientific System Design Inc., Mississauga, Ontario, Canada) with a total fluid dead space of approximately 3 ml. Slices were maintained at 30 to 32°C and constantly superfused at the rate of 2 ml/min. Solutions were applied to the slices by a peristaltic pump.
For patch-clamp experiments, individual slices (250 μm thick) were submerged in ACSF in the recording chamber at room temperature. The ACSF was perfused at a rate of approximately 1 ml/min.
In all experiments, unless otherwise specified, to isolate the NMDAR component, a modified ACSF (M-ACSF) containing low Mg2+ concentration (MgSO4 or MgCl2 were reduced to 0.2 mM) and the AMPA receptor blocker 2,3-dihydroxy-6-nitro-7-sulfamoyl-benzo[f]quinoxaline-2,3-dione (NBQX; 10 mM) were perfused for at least 20 minutes.
Field potential recording
Slices were visualized with a Wild M3B microscope (Heerbrugg, Switzerland). At the beginning of each recording, a concentric bipolar stimulating electrode (SNE-100X 50 mm long Elektronik-Harvard Apparatus GmbH, Crisel Instruments, Rome Italy) was positioned in the stratum radiatum for stimulation of Schaffer collateral pathway projections to CA1. An ACSF-filled glass micropipette (0.5 to 1 MΩ) was positioned 200 to 600 μm from the stimulating electrode for recording the orthodromically-evoked NMDAR component of field excitatory postsynaptic potentials (NMDA-fEPSPs). Stimuli consisted of 100-μs-long constant current square pulses, applied at 0.05 Hz. The intensity of the stimulus was adjusted in each experiment to evoke approximately 50% of the maximal field potential amplitude without appreciable population spike contamination. Evoked responses were monitored online and stable baseline responses were recorded for at least 10 minutes. Only the slices that showed stable NMDA-fEPSP amplitudes were included in the experiments. To analyze the timecourse of the NMDA-fEPSPs slope, the recorded NMDA-fEPSPs were routinely averaged over 1 minute (N = 3). Experiments were performed in M-ACSF and averaged NMDA-fEPSPs (last 5 minutes of treatment or washout) were normalized to baseline values (5 minutes) prior to treatment. In the text, n refers to the number of slices analyzed/number of mice.
For the paired-pulse ratio (PPR) test, closely spaced consecutive stimuli (50 ms interval) were used, and PPR was calculated as the ratio between the NMDA-fEPSPs amplitude evoked by the second stimulus (A2) over the first (A1; A2/A1).
NMDA-fEPSPs were recorded and filtered (1 kHz) with an Axopatch 200 A amplifier (Axon Instruments, CA, USA) and digitized at 10 kHz with an A/D converter (Digidata 1322A, Axon Instruments). Data were stored on a computer using pClamp 9 software (Axon Instruments) and analyzed offline with the Clampfit 9 program (Axon Instruments).
Neurons were visualized at 640 × with Nomarski optics with an upright Zeiss (Thornwood, NY, USA) Axioscope microscope. Patch-clamp recordings were obtained using glass electrodes (3 to 4 MΩ) filled with the following (in mM): CsMeSO4 135, CsCl 4, MgCl2 2, 2-[4-(2-hydroxyethyl)piperazin-1-yl]ethanesulfonic acid (HEPES) 10, MgATP 2, NaGTP 0.3, (1,2-bis(o-aminophenoxy)ethane-N,N,N',N'-tetraacetic acid (BAPTA) 5 (pH 7.3, with CsOH). Neurons were clamped at −70 mV and perfused with M-ACSF. NMDA currents in standard ACSF were recorded at positive potential to remove Mg block (10 mV) using the following solution (in mM): CsCl 130, MgCl2 2, HEPES 10, MgATP 2, NaGTP 0.3, BAPTA 5 (pH 7.3, with CsOH).
Membrane currents, recorded with a patch-clamp amplifier (Axopatch 200A; Molecular Devices, Foster City, CA, USA), were filtered at 2 kHz, digitized (10 kHz), and acquired with pClamp 9 software (Molecular Devices, Sunnyvale CA, USA). Excitatory postsynaptic currents (EPSCs) were evoked in CA1 pyramidal neurons by electrical stimulation with theta glass tubes pulled to a final tip diameter of 10 to 20 μm and filled with external solution. Stimulating electrodes were placed in the stratum radiatum to activate the Schaffer collateral pathway projecting to CA1. NMDA-EPSCs were evoked by stimulating at 5 to 50 V for 150 to 300 μs every 20 s. Recorded EPSCs were routinely averaged over 1 minute (N = 3) to analyze the timecourse of EPSC amplitude. Averaged NMDA-EPSCs (last 5 minutes of treatment or washout) were normalized to baseline values (5 minutes) prior to treatment. Stable EPSCs were monitored for at least 10 minutes before applying CX3CL1 and successively monitored during slice exposure to CX3CL1 (5 nM, a concentration close to the IC50 value for synaptic depression of AMPA mediated responses and to the concentration that inhibits NMDA-dependent LTP [15–17]. Data were analyzed offline with Clampfit 9 (Axon Instruments).
Glia and neuron primary cultures
Primary cortical glial cells were prepared from 0 to 2-day-old mice. Cerebral cortices were chopped and digested in 30 U/ml papain for 40 minutes at 37°C followed by gentle trituration. The dissociated cells were washed, suspended in Dulbecco’s modified Eagle medium (DMEM) with 10% fetal bovine serum (FBS) (Invitrogen, Life Technologies, Monza, Italy) and 2 mM l-glutamine and plated at a density of 9 to 10 × 105 in 175 cm2 cell culture flasks. At confluence (11 days in vitro), glial cells were plated (5.0 × 105 cells/cm2) on dishes coated with poly-l-lysine (100 μg/ml) in DMEM supplemented with 10% FBS, 100 U/ml penicillin, 0.1 mg/ml streptomycin. To detach and collect microglial cells, glial cells at confluence (11 days in vitro) were shaken for 2 h at 37°C. These procedures gave almost pure microglia (<2% astrocyte contamination) and astrocytes cell population (4% to 6% of microglia contamination), as verified by staining for glial fibrillary acidic protein (GFAP) and isolectin IB4.
Cortical neuronal cultures were prepared from newborn C57BL/6 mice (P0 to P1). Cerebral cortex were chopped and digested in 20 U/ml papain for 40 minutes at 37°C. Cells (13 × 104 cells/cm2) were plated on dishes coated with poly-l-lysine (100 μg/mL) in basal medium Eagle (BME) supplemented with 1 mM sodium pyruvate, 30 mM glucose, 0.1% Mito™ serum extender, 10% FBS, 100 U/mL penicillin, 0.1 mg/mL streptomycin and 10 mM HEPES-NaOH (pH 7.4). After 4 h the medium was changed with Neurobasal medium supplemented with 1 mM glutamine, 0.1% Mito™ serum extender, 2.5% B27, 100 U/ml penicillin and 0.1 mg/mL streptomycin. After 2 days, AraC (5 μM) was added to avoid the growth of glial cells. The percentage of neuronal cells obtained is 80% to 90%, as determined with β-tubulin III staining. Cultures were used after 10 to 11 days.
Measurement of d-serine by liquid chromatography and mass spectrometry (MS) analysis
Mixed glia, microglia and neuronal cultures at 11 days old were pretreated in M-ACSF for 40 minutes and stimulated for either 20 minutes, 2 h and 20 minutes and 4 h with CX3CL1 10 nM or vehicle. After this time, media were collected, centrifuged at 4°C for 10 minutes at high speed, and the resulting supernatants were kept to −20°C until use. Cells remaining in the dish were analyzed for protein content with a BCA assay (Pierce, Euroclone Pero, Italy).
Aliquots of the culture medium was derivatized according to the method described by Berna and Ackermann . Briefly, samples (25 μl) were incubated with 200 mM (pH 7.5) sodium bicarbonate solution and 10 μl of 1% Marfey’s reagent (w/v in acetone) at 60°C for 1h.
Next, the samples were evaporated to dryness at 60°C under a stream of nitrogen, and the dried residues were reconstituted with 12.5% methanol in 15 mM ammonium acetate. The samples were centrifuged at 600 g for 5 minutes and the supernatants diluted with 200 μl of mobile phase. Injections of 20 μl were performed for liquid chromatography-tandem mass spectrometry (LC-MS/MS) analysis. Marfey’s adducts of D standard mixture were prepared by appropriate dilution of the 100 μg/ml stock solution of d-serine in high-performance liquid chromatography (HPLC)-grade water and following the same derivatization procedure.
The LC-MS/MS system consisted of a PerkinElmer 200 Series binary pump and autosampler (PerkinElmer, Norwalk, CT, USA) and an SCIEX API2000MS/MS triple quadrupole mass spectrometer including a Turbolon Spray® ionization source (Applied Biosystem-MDS SCIEX, Thornhill, Ontario, Canada).
Chromatographic separation was performed on a Synergi Polar RP column (150 × 2.0 mm, 4 μm), protected by a guard column with identical packing material (4 × 2.0 mm; Phenomenex, Torrance, CA, USA) The mobile phase consisted of a linear gradient (30% to 70% with respect to acetonitrile) formed by combination of 5 mM ammonium formate buffer in water (pH 4.0, eluent A) and acetonitrile (eluent B) at a flow rate of 0.2 ml/min.
d-Serine derivatives were detected using multiple reaction monitoring (MRM) in negative ionization mode. Selected ion masses of the protonated precursors and fragmented ions (m/z) were 359.1 > 192. Chromatographic peaks were integrated using Analyst™ software (version 1.4.1, SCIEX). The detection limits (LOD) and quantification limits (LOQ) for d-serine were 1.71 ng/ml and 5.18 ng/ml respectively. The Marfey’s derivated isobaric compounds l-Ser and d-Ser (2,4-dinitro-phenyl-5-l-alanine amide- (DNPA-)l-Ser and DNPA-d-Ser) were well resolved chromatographically as shown in Additional file 1: Figure S1. An example of the blank samples (control M-ACSF) is shown in Additional file 2: Figure S2, where no signal corresponding to DNPA-l-Ser or DNPA-d-Ser are present.
The values were reported as mean ± SEM. Unless otherwise specified, data values refer to number of slices/number of animals analyzed. Where appropriate, t tests or one-way analysis of variance (ANOVA) were used. Since in all experiments data passed the normality and the equal variance tests, we performed parametric ANOVA followed by Tukey or Holm-Sidak multiple-comparison test (Sigma Plot, 11.0 software). If not specified, P values refer to ANOVA post hoc analyses.
CX3CL1 (human, Peprotech Inc. Rocky Hill, NJ, USA), 7-(2-phenylethyl)-5-amino-2-(2-furyl)-pyrazolo-[4,3-e]-1,2,4-triazolo[1,5-c]pyrimidine (SCH58261, stock solution 10 mM in dimethylsulfoxide (DMSO)), triazoloquinazoline (CGS15943, stock solution 5 mM in DMSO) and 1,3-dipropyl-8-cyclopentylxanthine (DPCPX stock solution 5 mM in DMSO) by Tocris Bioscience, Bristol, UK. 3-Propyl-6-ethyl-5-[(ethylthio)carbonyl]-2 phenyl-4-propyl-3-pyridine carboxylate (MRS1523, stock solution 10 mM), catalase, d-amino acid oxidase (DAAO), Marfey’s reagent (Nα-(2,4-dinitro-5-fluophenyl)-l-alaninamide), ammonium formate and Minocycline (stock solution 20 mM) from Sigma-Aldrich (Milan, Italy). NBQX (stock solution 20 mM), 5,7-dicholorokynurenic acid (DCKA, stock solution 750 μM in 1 eq. NaOH) and d-serine (stock solution 10 mM) by Ascent Scientific, Bristol, UK. 5-(6-Amino-2-(phenethylthio)-9H-purin-9-yl)-N-ethyl-3,4-dihydroxytetrahydrofuran-2-carboxamide (VT7, stock solution 10 mM in DMSO). Adenosine deaminase (ADA, Roche, Germany). Acetonitrile, methanol, both gradient grades were purchased from Merck (Darmstadt, Germany). Ultrapure water was prepared using a Millu-Q system (Millipore, MA, USA).
Drugs were dissolved in ACSF just before application.
CX3CL1 increases hippocampal NMDA responses
To investigate whether CX3CL1 influences NMDA-mediated synaptic transmission in hippocampal CA1 region, we recorded the NMDAR component of the fEPSPs (NMDA-fEPSPs) elicited in the CA1 stratum radiatum of mouse hippocampal slices by electrical stimulation of the Schaffer collateral (at 0.05 Hz). To isolate the NMDA component of the fEPSPs slices were treated with the AMPA receptor blocker NBQX (10 μM) and with low (0.2 mM) magnesium . In control slices, synaptic activity was stable for at least 30 minutes (not shown). We challenged the slices with CX3CL1 at concentrations of 5 nM. In the majority of the experiments (25 out of 35 slices tested, 28 mice; Figure 1A) bath application of CX3CL1 for 20 minutes induced a short-term potentiation (STP) of synaptic transmission. The potentiation of the NMDA-fEPSPs slope developed within 5 minutes of CX3CL1 application was 1.22 ± 0.03 of baseline (from 1.92 to 1.01 in different experiments, measured here and thereafter after 20 minutes of treatment, P <0.05) and was followed by partial recovery (to 1.15 ± 0.01 of baseline, P <0.05, measured here and thereafter at 20 minutes of CX3CL1 withdrawal) with a few exceptions where full recovery was observed. To exclude the possibility that CX3CL1 treatment induces a change in presynaptic cell excitability, such as the recruitment of more presynaptic fibers by the same stimulus, changes in the amplitude of extracellular fiber volley (an index of presynaptic excitation) were monitored by recording evoked fEPSPs during CX3CL1 application. As shown in Additional file 3: Figure S3A, in a subset of slices where the potentiating effect of CX3CL1 was maximal (41.68 ± 0.05 of baseline, n = 5, P <0.05) the amplitude of the afferent volley did not change after treatment with CX3CL1 (P = 0.45, paired t test).
Patch-clamp experiments were carried out to measure CX3CL1-mediated modulation of NMDA current at the single cell level. Whole-cell recordings of NMDA-EPSCs were performed in CA1 pyramidal neurons in acute slices while repeatedly stimulating Schaffer collateral axons. CX3CL1 treatment caused an increase in NMDA-EPSC peak amplitude (to 1.25 ± 0.03 P < 0.05 vs baseline) that recovered upon withdrawal (to 1.06 ± 0.04 P >0.05 vs baseline, Figure 1B, five slices/five mice). These results confirmed the CX3CL1-mediated potentiation of NMDA responses also at the single cell level.
Paired pulse facilitation (PPF) ratio is not altered by CX3CL1 application
To analyze if CX3CL1 potentiates NMDA-fEPSPs by altering presynaptic glutamate release, we performed studies of short-term plasticity, that is, paired-pulse ratio (PPR) measurements. The PPR, which is the ratio of the amplitude of the second response vs the first, depends on the probability of vesicular release at synapse and its variation is generally associated with changes in transmitter release probability .
To evaluate PPR values we stimulated Schaffer collateral pathway projections to CA1 at 50 ms intervals. As shown in Additional file 3: Figure S3B, PPR was 1.53 ± 0.017 and 1.54 ± 0.026 before and after 20 min of CX3CL1 treatment (6 slices/4 mice, P = 0.74, paired t test), respectively.
Presynaptic release of Glu can be affected by removal of Mg2+ from the external solution, changing the competition between Mg2+ and Ca2+ at terminal endings and altering PPR mechanisms . To investigate this possibility we repeated the PPR measurements in whole-cell experiments where the NMDA current were isolated by depolarizing the cell in a standard ACSF medium. As shown in Additional file 3: Figure S3C, the PPR measured in this condition was 1.43 ± 0.08 and 1.44 ± 0.09 before and after 20 minutes of CX3CL1 treatment, (5 slices/5 mice, P = 0.81, paired t test). These data indicated that under our experimental conditions, CX3CL1 treatment did not cause obvious changes in presynaptic release probability, confirming the postsynaptic nature of the potentiation of NMDA-fEPSPs, in line with our previous findings [15, 44].
CX3CL1-mediated effects require the presence of CX3CR1 on microglial cells
To demonstrate that the effects of CX3CL1 were indeed mediated by CX3CR1, experiments were performed on CX3CR1GFP/GFP mice where the murine CX3CR1 gene was replaced with the cDNA encoding EGFP (Jung et al. ). Application of CX3CL1 for 20 minutes to CX3CR1GFP/GFP hippocampal slices (Figure 2A, seven slices/three mice) failed to induce any obvious basal NMDA-fEPSPs slope change (P > 0.05). These findings clearly show that CX3CL1-induced effects on NMDA-fEPSPs were mediated through CX3CR1 activation.
Since CX3CR1 is expressed on microglial cells [5, 6], we wondered whether microglial activation was required for CX3CL1-mediated STP of NMDA-fEPSPs. For this purpose we treated hippocampal slices with a broad-spectrum tetracycline antibiotic, minocycline, known to inhibits microglial activation [45–47].
As shown in Figure 2B, in the presence of minocycline (20 μM, 1 h preincubation), the application of CX3CL1 did not significantly affect the NMDA-fEPSPs (P > 0.5, eight slices/two mice), demonstrating a microglia-driven chemokine effect.
CX3CL1-mediated NMDAR potentiation is mediated by ARs
We have previously shown that CX3CL1 treatment induces the release of adenosine from microglia  and that CX3CL1-mediated modulation of synaptic transmission and plasticity involves AR activity [17, 48]. In addition, it is known that AR activity in the hippocampus modulates NMDA receptor functioning . For all these reasons we investigated whether CX3CL1 effects on NMDARs require AR activity. We first treated hippocampal slices with the broad-spectrum AR antagonist CGS15943. The applications of CGS15943 (1 μM) abolished CX3CL1-mediated STP of NMDA-fEPSPs (Figure 3A, P > 0.05 vs baseline, nine slices/four mice) indicating that the activity of ARs is indeed involved in CX3CL1 effects.
To disclose the specific role of distinct AR subtypes, we performed additional experiments with selective A1R, A2AR and A3R antagonists (Figure 3B-D).
Specifically, the A1R antagonist DPCPX (25 nM) failed to prevent CX3CL1-mediated modulation of NMDAR, as the NMDA-fEPSPs slope increased during CX3CL1 treatment (to 1.25 ± 0.01, P < 0.05 vs baseline, P > 0.05 vs CX3CL1 alone) and remained high upon withdrawal (to 1.25 ± 0.04 P < 0.05 vs baseline, Figure 3B, nine slices/five mice). Similarly, the specific A3R antagonist MRS1523 (100 nM) was unable to affect the action of CX3CL1 that elicited a significant increase in NMDA-fEPSPs slope (to 1.23 ± 0.01, P < 0.05 vs baseline, P > 0.05 vs CX3CL1 alone) partially recovering upon withdrawal (1.12 ± 0.01, P < 0.05 vs baseline, Figure 3C, ten slices/five mice).
Conversely, when slices were treated with the selective A2AR antagonist SCH58261 (10 nM), CX3CL1 was unable to affect NMDA-fEPSPs slope (Figure 3D, P > 0.05 vs baseline P < 0.01 vs CX3CL1 alone, six slices/three mice), indicating that A2AR activity is associated with CX3CL1 effects on NMDAR-dependent basal transmission.
The role of ARs in CX3CL1 effects was further investigated by means of mice selectively lacking AR subtypes. As shown in Figure 4A application of CX3CL1 in A1R−/− mice increased NMDA-fEPSPs slope (to 1.14 ± 0.01, P < 0.05 vs baseline) that partially recovered after washout (to 1.04 ±0.02, P > 0.05 vs baseline, ten slices/three mice). Similar results were obtained in A3R−/− mice, where CX3CL1 elicited a significant increase of NMDA-fEPSPs slope (to 1.11 ± 0.01, P < 0.05 vs baseline) that recovered upon withdrawal (to 1.02 ± 0.01, P > 0.05 to baseline, Figure 4B, ten slices/two mice). Interestingly, in accordance with pharmacological data, in A2AR deficient mice (A2AR−/−) CX3CL1 was unable to affect NMDA-fEPSPs. (P > 0.05, vs baseline, 11 slices/3 mice, Figure 4C), thus pointing to an essential role of A2AR activity in the CX3CL1 effect. To further support this observation, we tested whether a selective A2AR agonist, VT7 (50 nM), was able to mimic CX3CL1 effect. The results in Figure 5A demonstrate that in the presence of adenosine deaminase (ADA, 1 U/ml), which removes ambient adenosine , VT7 induced an increase of NMDA-fEPSPs slope (to 1.18 ± 0.01, P < 0.05 vs baseline, nine slices/two mice) that did not recover after washout (to 1.15 ± 0.01, P < 0.05 vs baseline).
Considered together, our findings indicate that the influence of CX3CL1 on NMDARs is mediated by the A2AR activity.
d-serine is involved in CX3CL1-dependent modulation of NMDARs
Recent evidence indicates that d-serine serves as indispensable cofactor at the glycine binding site of NMDARs representing a new and important glia-derived neuromodulatory factor . In fact, in glial cells, d-serine is synthesized and metabolized endogenously by the enzymes serine racemase (SR)  and d-amino acid oxidase (DAAO) , respectively.
To investigate whether d-serine is involved in CX3CL1-mediated modulation of NMDARs, we first treated the slices with the selective NMDAR glycine-site antagonist 5,7-dichlorokynurenic acid (DCKA) at a concentration (750 nM) known to reduce NMDA responses by around 25%  and able to prevent d-serine mediated increase of NMDA-fEPSPs slope (n = 7, data not shown). At this concentration, DCKA abolished CX3CL1 effects on NMDA-fEPSPs (P > 0.05 vs baseline, eight slices/four mice, Figure 6A).
To disclose a possible d-serine versus glycine coagonist requirement, we treated the slices with DAAO (0.1 U/ml). Excess catalase (300 U/ml) was added in the solution in order to avoid the possibility of hydrogen peroxide production from the enzymatic degradation of d-serine by DAAO. Under this condition, DAAO completely prevented CX3CL1 action (P > 0.05 vs baseline, ten slices/four mice, Figure 6B), indicating that d-serine is necessary. To further confirm the involvement of d-serine in the modulation of NMDARs by CX3CL1, we applied exogenous d-serine (10 μM, six slices/four mice, Figure 6C) to hippocampal slices. As shown in Figure 6C, d-serine produced an increase in NMDA-fEPSPs slope reaching a plateaux effect within 20 minutes (up to 64.4 ± 0.01 after 40 minutes treatment, P < 0.05 vs baseline). Subsequent coapplication of CX3CL1 failed to further increase NMDA-fEPSPs slope (P > 0.05 vs d-serine alone), indicating that saturation of the glycine site by d-serine interferes with chemokine action.
Since we have demonstrated that the CX3CL1 effect is prevented by hampering both d-serine and A2AR functions, we investigated whether the two pathways share some common mechanisms of action. For this reason we applied the A2AR agonist VT7 (in the presence of ADA, 1 U/ml) while partially blocking the NMDAR d-serine site by DCKA. In this condition, VT7 failed to increase NMDA-fEPSPs slope (P > 0.05 vs baseline, Figure 5B, 11 slices/3 mice). In addition, slices pretreatment with DAAO (0.1 U/ml, in the presence of catalase, 300 U/ml, and ADA, 1 U/ml) inhibits VT7 action (>0.05 vs baseline, Figure 5C, seven slices/three mice). Taken together this evidence suggests that NMDAR modulation mediated by A2AR requires d-serine.
CX3CL1 and VT7 stimulate the release of d-serine from glia cells
To further investigate the possible source of d-serine in CX3CL1-induced NMDAR modulation, we measured d-serine levels in glia-conditioned medium. The control medium (M-ACSF) did not contain d-serine, as it is shown in Additional file 2: Figure S2.
Primary cortical glial cells and isolated microglial cell populations were stimulated with CX3CL1 (10 nM) for different times (20 minutes, 2 h and 20 minutes or 4 h). After stimulation, mass spectrometry was performed on media samples.
Treatment of both primary purified microglia and mixed glia with CX3CL1 resulted in a large increase in d-serine in the medium (Figure 7). In particular, in microglial cells CX3CL1 induced a significant increase in d-serine release at all the incubation times considered (1.53 ± 0.08 after 20 minutes, 1.26 ± 0.07 after 2 h and 20 minutes and 2.63 ± 0.80 after 4 h, P < 0.05 in all cases vs untreated, n = 8, Figure 7A). Similarly, CX3CL1 treatment augmented d-serine level in the medium of mixed glia (1.76 ± 0.19 after 20 minutes, 1.66 ± 0.11 after 2 h and 20 minutes and 1.52 ± 0.24 after 4 h, P < 0.05 in all cases vs untreated, n = 8, Figure 7B).
We then tested whether also the A2AR agonist VT7 was able to modulate the release of d-serine from glia. For this purpose we stimulated the cells with VT7 (50 nM) in the continuous presence of adenosine deaminase (ADA, 1 U/ml). As for CX3CL1, the A2AR agonist was able to induce an increment in the basal level of d-serine. Specifically, VT7 treatment produced an increase in d-serine release in both primary purified microglia (up to: 1.28 ± 0.13 after 20 minutes, 1.38 ± 0.10 after 2 h and 20 minutes and 1.60 ± 0.30 after 4 h, P < 0.05 in all cases vs untreated, n = 9, Figure 7C) and mixed glia medium (up to: 1.53 ± 0.10 after 20 minutes, 1.37 ± 0.06 after 2 h and 20 minutes and 1.47 ± 0.12 after 4 h, P < 0.05 in all cases vs untreated, n = 12, Figure 7D), respectively. Interestingly, the control basal level of d-serine in purified microglia medium was unchanged at different time points, whereas in mixed glia it accumulates upon time, and it had similar values (at 20 minutes, both in M-ACSF or M-ACSF plus ADA, P >0.05 for all cases). In addition, the level of basal d-serine released by mixed glia or microglia was in the order of 10 fmol/cell, accordingly to previously reported values .
We further tested the ability of VT7 to induce the release of d-serine form neurons in the presence of ADA. During treatment, no variation in the basal level of d-serine was observed, at all time points considered (P > 0.05 vs untreated, n = 12). Notably, the basal level of d-serine released by neurons was much lower compared to glia (at 20 minutes: 37.24 ± 7.02 ng/mg of protein, n = 12).
The main finding of the present study is that NMDAR function, in CA1 hippocampal region, is potentiated by CX3CL1 application. The activation of the glial A2AR and the release of the NMDAR coagonist d-serine are likely major causative factors for the observed NMDA potentiation. Interestingly this effect is postsynaptic in nature, depends on microglia and requires the presence of CX3CR1. Specifically, the parameter related to changes in the probability of vesicular release at the synapse, such as PPR, was not affected by CX3CL1, indicating that the chemokine did not potentiate NMDA-fEPSPs by altering presynaptic glutamate release (see also [15, 44]). In addition, the use of genetically modified mice lacking CX3CR1 or inhibiting microglia function by minocycline treatment prevented CX3CL1-mediated potentiation of NMDAR function.
A2AR activity is involved in CX3CL1 effect
It is established that adenosine acts as neuromodulator of NMDAR function; in particular A2ARs exert a facilitatory role on NMDARs [55, 56]. Nevertheless, the consequences of A2AR activation on synaptic transmission in physiological conditions of adenosine release remained elusive. Since the ambient level of adenosine is sufficient to activate inhibitory A1R but not facilitatory A2AR, possibly due to differences in affinity , it is believed that specific stimulation such as high-frequency bursts is needed to increase the level of adenosine to values able to activate A2AR . Indeed, we have previously demonstrated that stimulation of microglial cells by CX3CL1 induces an increase in extracellular level of adenosine .
Here, we reported that CX3CL1-mediated activation of A2AR influences the NMDA-mediated component of excitatory synaptic transmission. In particular, the specific A2AR blocker SCH58261, as well as the genetic ablation of A2AR, prevented the short-term potentiation of NMDA fEPSPs induced by CX3CL1. In addition, the specific A2AR agonist VT7 was able to mimic CX3CL1 effect, producing a similar potentiation of NMDA-fEPSPs.
d-serine is essential for CX3CL1-mediated potentiation of NMDA-fEPSPs
It is well established that d-serine act as an essential coagonist of NMDAR. The production of d-serine in the mammalian brain results from the activity of SR, an enzyme that converts l-serine into d-serine . Astrocytes synthesize and release d-serine , for instance following activation of AMPARs by glutamate released from nerve terminals [24, 60]. In contrast, scarce information is available on microglia derived d-serine. It has been reported that microglia express serine racemase [27–29] and release d-serine after activation with amyloid β-peptide .
We demonstrated that d-serine is involved in CX3CL1-mediated potentiation of NMDA-fEPSPs because its action is prevented by: (i) the selective NMDAR antagonist of the glycine (and d-serine)-binding site DCKA, (ii) the enzymatic degradation of d-serine by DAAO, and (iii) the saturation of the coagonist site by d-serine.
In addition, mass spectrometry analysis revealed that treatment of primary mixed glial cells and purified microglial population with CX3CL1 induces a significant increase of d-serine release in the extracellular medium. The glial population used for these studies was derived from cerebral cortices and we are aware that microglial phenotypes differ across brain regions and ages [61, 62], so that results from these preparation cannot be directly transferred to hippocampal glial cells; nevertheless these data strongly support a direct role of CX3CL1 in controlling d-serine release from glia, that need further investigation, and clearly demonstrate a basal release of d-serine from microglial cells that can be further increased by CX3CL1 treatment.
Overall, the evidence suggests that both A2AR activity and d-serine release are needed for CX3CL1-mediated potentiation of NMDA-fEPSPs. Are these factors interacting in some way? Our results point to a possible crosstalk between A2AR activity and d-serine release. First of all, at Schaffer collateral-CA1 synapses the A2AR agonist failed to increase NMDA-fEPSPs when the NMDA glycine site was partially blocked by DCKA, indicating an extracellular modulation (via d-serine binding) of NMDAR mediated by the activation of A2AR. It is unlikely that the partial block of the NMDAR extracellular site could mask a possible A2AR-mediated intracellular modulation of the receptor , the latter actually occurring at hippocampal mossy-CA3 synapse via calcium amplification signals . In addition, enzymatic degradation of d-serine by DAAO prevented the A2AR agonist mediated potentiation of NMDA-fEPSPs, supporting the d-serine requirement for VT7 effect.
Secondly, by means of mass spectrometry analysis, we have shown that primary glial cells and purified microglia are capable to release d-serine in the medium after stimulation with VT7. These observations suggest a direct role of A2AR in controlling the release of d-serine from glia that in turn can modulate NMDAR functions. To the best of our knowledge, this is the first report on adenosine-mediated release of d-serine from glia. A2AR are indeed expressed on microglia and astrocytes [49, 64, 65], usually coupled to Gs proteins, enhancing PKA or PKC activity [56, 58, 66]. Interestingly, PKC activity seems relevant in regulating SR activity and d-serine availability [67–69]. Since it has been reported that neuronal cells can release d-serine, with controversial functions on synaptic NMDAR [70, 71], we investigated whether VT7 stimulated d-serine release from neurons. The basal release of d-serine from neurons appeared markedly reduced compared to glia and the activation of neuronal A2AR was unable to further increase the extracellular d-serine levels, although we cannot exclude an indirect modulation of neuronal d-serine via other mediators released by CX3CL1-activated microglia.
We have previously demonstrated that CX3CL1 inhibits AMPA-mediated transmission and LTP expression [15, 17] while here we reported that CX3CL1 potentiates NMDAR. We speculate that the persistent CX3CL1-mediated potentiation of NMDA function and the consequent calcium increase could interfere with the complex mechanisms of LTP induction that depends not only by the precise amplitude but also by the duration of postsynaptic Ca2+ increase and by the recent history of synaptic activity. Indeed, it has been demonstrated that prior activation of NMDAR either by synaptic or pharmacological stimulation could effectively inhibit the subsequent LTP induction [72, 73].
Since in our experimental setting we recorded synaptic NMDAR blocking AMPAR component, it would be informative to investigate CX3CL1-mediated NMDAR modulation in a more physiological condition, where neuronal and glial AMPAR are activable.
Interestingly, the effect of CX3CL1 seems to be specific for the synaptic NMDARs that are exclusively gated by the coagonist d-serine . It has been reported that activation of synaptic NMDARs (NR2A-containing NMDARs) preferentially triggers cell survival pathways, whereas stimulation of the whole-cell population of NMDARs and/or selective activation of extrasynaptic NMDARs (NR2B-containing NMDARs) signals toxic stimuli ([74, 75], but see also ). Therefore, CX3CL1-mediated potentiation of synaptic NMDAR function can possibly contribute to the neuroprotective action of CX3CL1 described in different in vitro and in vivo conditions [11, 12, 14].
Future studies are warranted to discern the role and the precise mechanism of CX3CL1-mediated potentiation of NMDA-fEPSPs in both physiological and pathological condition, with particular attention to the sequence of mediators and cell types involved, namely neurons, astrocytes or microglia. Nevertheless, considering overall data, we can speculate that on microglial cells the activation of CX3CR1 triggers the release of adenosine that in turn, via A2AR activity, increases the release of d-serine from glia leading to a potentiation of NMDA function (Figure 8).
In summary, we have demonstrated a direct association between the effects of CX3CL1 on NMDAR activation and increased levels of d-serine and A2AR activity within the CA1 region of the hippocampus. The CX3CL1-CX3CR1 axis therefore represents a pathway for direct communication between neural cells and microglia.
Rostène W, Kitabgi P, Parsadaniantz SM: Chemokines: a new class of neuromodulator. Nat Rev Neurosci 2007, 8:895–903.
Réaux Le Goazigo A, Van Steenwinckel J, Rostène W, Mélik Parsadaniantz S: Current status of chemokines in the adult CNS. Prog Neurobiol 2013, 104:67–92.
Harrison LK, Jiang Y, Chen S, Xia Y, Maciejewski D, McNamara RK, Streit JW, Salafranca MN, Adhikari S, Thompson DA, Botti P, Bacon KB, Feng L: Role for neuronally derived fractalkine in mediating interactions between neurons and CX3CR1-expressing microglia. Proc Natl Acad Sci USA 1998, 95:10896–10901.
Hatori K, Nagai A, Heisel R, Ryu JK, Kim SU: Fractalkine and fractalkine receptors in human neurons and glial cells. J Neurosci Res 2002, 69:418–426.
Cardona AE, Pioro EP, Sasse ME, Kostenko V, Cardona SM, Dijkstra IM, Huang D, Kidd G, Dombrowski S, Dutta R, Lee JC, Cook DN, Jung S, Lira SA, Littman DR, Ransohoff RM: Control of microglial neurotoxicity by the fractalkine receptor. Nat Neurosci 2006, 9:917–924.
Jung S, Aliberti J, Graemmel P, Sunshine MJ, Kreutzberg GW, Sher A, Littman DR: Analysis of fractalkine receptor CX(3)CR1 function by targeted deletion and green fluorescent protein reporter gene insertion. Mol Cell Biol 2000, 20:4106–4114.
Wolf Y, Yona S, Kim KW, Jung S: Microglia, seen from the CX3CR1 angle. Front Cell Neurosci 2013, 7:26.
Hughes PM, Botham MS, Frentzel S, Mir A, Perry VH: Expression of fractalkine (CX3CL1) and its receptor, CX3CR1, during acute and chronic inflammation in the rodent CNS. Glia 2002, 37:314–327.
Sunnemark D, Eltayeb S, Nilsson M, Wallström E, Lassmann H, Olsson T: CX3CL1 (fractalkine) and CX3CR1 expression in myelin oligodendrocyte glycoprotein-induced experimental autoimmune encephalomyelitis: kinetics and cellular origin. J Neuroinflammation 2005, 2:17–31.
D'Haese JG, Friess H, Ceyhan GO: Therapeutic potential of the chemokine-receptor duo fractalkine/CX3CR1: an update. Expert Opin Ther Targets 2012, 16:613–618.
Limatola C, Lauro C, Catalano M, Ciotti MT, Bertollini C, Di Angelantonio S, Ragozzino D, Eusebi F: Chemokine CX3CL1 protects rat hippocampal neurons against glutamate-mediated excitotoxicity. J Neuroimmunol 2005, 166:19–28.
Lauro C, Di Angelantonio S, Cipriani R, Sobrero F, Antonilli L, Brusadin V, Ragozzino D, Limatola C: Activity of adenosine receptors type 1 is required for CX3CL1-mediated neuroprotection and neuromodulation in hippocampal neurons. J Immunol 2008, 180:7590–7596.
Lauro C, Cipriani R, Catalano M, Trettel F, Chece G, Brusadin V, Antonilli L, van Rooijen N, Eusebi F, Fredholm BB, Limatola C: Adenosine A1 receptors and microglial cells mediate CX3CL1-induced protection of hippocampal neurons against Glu-induced death. Neuropsychopharmacology 2010, 35:1550–1559.
Cipriani R, Villa P, Chece G, Lauro C, Paladini A, Micotti E, Perego C, De Simoni MG, Fredholm BB, Eusebi F, Limatola C: CX3CL1 is neuroprotective in permanent focal cerebral ischemia in rodents. J Neurosci 2011, 31:16327–16335.
Ragozzino D, Di Angelantonio S, Trettel F, Bertollini C, Maggi L, Gross C, Charo IF, Limatola C, Eusebi F: Chemokine fractalkine/CX 3 CL1 negatively modulates active glutamatergic synapses in rat hippocampal neurons. J Neurosci 2006, 26:10488–10498.
Bertollini C, Ragozzino D, Gross C, Limatola C, Eusebi F: Fractalkine/CX3CL1 depresses central synaptic transmission in mouse hippocampal slices. Neuropharmacology 2006, 51:816–821.
Maggi L, Trettel F, Scianni M, Bertollini C, Eusebi F, Fredholm BB, Limatola C: LTP impairment by fractalkine/CX(3)CL1 in mouse hippocampus is mediated through the activity of adenosine receptor type 3 (A(3)R). J Neuroimmunol 2009, 215:36–42.
MacDermott AB, Mayer ML, Westbrook GL, Smith SJ, Barker JL: NMDA-receptor activation increases cytoplasmic calcium concentration in cultured spinal cord neurones. Nature 1986, 321:519–522.
Cull-Candy S, Brickley S, Farrant M: NMDA receptor subunits: diversity, development and disease. Curr Opin Neurobiol 2001, 11:327–335.
Hollmann M, Heinemann S: Cloned glutamate receptors. Annu Rev Neurosci 1994, 17:31–108.
Johnson JW, Ascher P: Glycine potentiates the NMDA response in cultured mouse brain neurons. Nature 1987, 325:529–531.
Matsui T, Sekiguchi M, Hashimoto A, Tomita U, Nishikawa T, Wada K: Functional comparison of D -serine and glycine in rodents: the effect on cloned NMDA receptors and the extracellular concentration. J Neurochem 1995, 65:454–458.
Papouin T, Ladépêche L, Ruel J, Sacchi S, Labasque M, Hanini M, Groc L, Pollegioni L, Mothet JP, Oliet SH: Synaptic and extrasynaptic NMDA receptors are gated by different endogenous coagonists. Cell 2012, 150:633–646.
Schell MJ, Brady RO Jr, Molliver ME, Snyder SH: D -serine as a neuromodulator: regional and developmental localization in rat brain glia resemble NMDA receptors. J Neurosci 1997, 17:1604–1615.
Wu SZ, Bodles AM, Porter MM, Griffin WS, Basile AS, Barger SW: Induction of serine racemase expression and D -serine release from microglia by amyloid beta-peptide. J Neuroinflammation 2004, 1:2.
Williams SM, Diaz CM, Macnab LT, Sullivan RK, Pow DV: Immunocytochemical analysis of D -serine distribution in the mammalian brain reveals novel anatomical compartmentalizations in glia and neurons. Glia 2006, 53:401–411.
Sasabe J, Chiba T, Yamada M, Okamoto K, Nishimoto I, Matsuoka M, Aiso S: D -serine is a key determinant of glutamate toxicity in amyotrophic lateral sclerosis. EMBO J 2007, 26:4149–5159.
Wang W, Barger SW: Cross-linking of serine racemase dimer by reactive oxygen species and reactive nitrogen species. J Neurosci Res 2012, 90:1218–1229.
Hayashi Y, Ishibashi H, Hashimoto K, Nakanishi H: Potentiation of the NMDA receptor-mediated responses through the activation of the glycine site by microglia secreting soluble factors. Glia 2006, 53:660–668.
Block ML, Zecca L, Hong JS: Microglia-mediated neurotoxicity: uncovering the molecular mechanisms. Nat Rev Neurosci 2007, 8:57–69.
Flavin MP, Zhao G, Ho LT: Microglial tissue plasminogen activator (tPA) triggers neuronal apoptosis in vitro . Glia 2000, 29:347–354.
Jarvis CR, Xiong ZG, Plant JR, Churchill D, Lu WY, MacVicar BA, MacDonald JF: Neurotrophin modilation of NMDA receptors in cultures murine and isolated rat neurons. J Neurophysiol 1997, 78:2363–2371.
Nakanishi H: Microglial functions and proteases. Mol Neurobiol 2003, 27:163–176.
Yang S, Liu ZW, Qiao HF, Zhou WX, Zhang YX: Interleukin-1 b enhances NMDA receptor-mediated current but inhibits excitatory transmission. Brain Res 2005, 1034:172–179.
Deiva K, Geeraerts T, Salim H, Leclerc P, Héry C, Hugel B, Freyssinet JM, Tardieu M: Fractalkine reduces N -methyl- D -aspartate-induced calcium flux and apoptosis in human neurons through extracellular signal-regulated kinase activation. Eur J Neurosci 2004, 20:3222–3232.
Cook DN, Cook DN, Chen SC, Sullivan LM, Manfra DJ, Wiekowski MT, Prosser DM, Vassileva G, Lira SA: Generation and analysis of mice lacking the chemokine fractalkine. Mol Cell Biol 2001, 21:3159–3165.
Johansson B, Halldner L, Dunwiddie TV, Masino SA, Poelchen W, Gimenez-Llort L, Escorihuela RM, Fernandez-Teruel A, Wiesenfeld-Hallin Z, Xu XJ, Hardemark A, Betsholtz C, Herlenius E, Fredholm BB: Hyperalgesia, anxiety, and decreased hypoxic neuroprotection in mice lacking the adenosine A1 receptor. Proc Natl Acad Sci USA 2001, 98:9407–9412.
Salvatore CA, Tilley SL, Latour AM, Fletcher DS, Koller BH, Jacobson MA: Disruption of the A(3) adenosine receptor gene in mice and its effect on stimulated inflammatory cells. J Biol Chem 2000, 275:4429–4434.
Chen JF, Huang Z, Ma J, Zhu J, Moratalla R, Standaert D, Moskowitz MA, Fink JS, Schwarzschild MA: A(2A) adenosine receptor deficiency attenuates brain injury induced by transient focal ischemia in mice. J Neurosci 1999, 19:9192–9200.
Berna MJ, Ackermann BL: Quantification of serine enantiomers in rat brain microdialysate using Marfey’s reagent and LC/MS/MS. J Chromatogr 2007, 846:359–363.
Neagu B, Strominger NL, Carpenter DO: Contribution of NMDA receptor-mediated component to the EPSP in mouse Schaffer collateral synapses under single pulse stimulation protocol. Brain Res 2008, 1240:54–61.
Zucker RS: Short-term synaptic plasticity. Ann Rev Neurosci 1989, 12:13–31.
Maggi L, Sola E, Minneci F, Le Magueresse C, Changeux JP, Cherubini E: Persistent decrease in synaptic efficacy induced by nicotine at Schaffer collateral-CA1 synapses in the immature rat hippocampus. J Physiol 2004, 559:863–874.
Maggi L, Scianni M, Branchi I, D’Andrea I, Lauro C, Limatola C: CX(3)CR1 deficiency alters hippocampal-dependent plasticity phenomena blunting the effects of enriched environment. Front Cell Neurosci 2011, 5:22.
Suzuki H, Sugimura Y, Iwama S, Suzuki H, Nobuaki O, Nagasaki H: Minocycline prevents osmotic demyelination syndrome by inhibiting the activation of microglia. J Am Soc Nephrol 2010, 21:2090–2098.
Yrjanheikki J, Keinanen R, Pellikka M, Hokfelt T, Koistinaho J: Tetracyclines inhibit microglial activation and are neuroprotective in global brain ischemia. Proc Natl Acad Sci USA 1998, 95:15769.
Tikka TM, Koistinaho JE: Minocycline provides neuroprotection against N -methyl- D -aspartate neurotoxicity by inhibiting microglia. J Immunol 2001, 166:7527–7533.
Piccinin S, Di Angelantonio S, Piccioni A, Volpini R, Cristalli G, Fredholm BB, Limatola C, Eusebi F, Ragozzino D: CX3CL1-induced modulation at CA1 synapses reveals multiple mechanisms of EPSC modulation involving adenosine receptor subtypes. J Neuroimmunol 2010, 224:85–92.
Sebastião AM, Ribeiro JA: Tuning and fine-tuning of synapses with adenosine. Curr Neuropharmacol 2009, 7:180–194.
Lopes LV, Cunha RA, Kull B, Fredholm BB, Ribeiro JA: Adenosine A 2A receptor facilitation of hippocampal synaptic transmission is dependent on tonic A 1 receptor inhibition. Neuroscience 2002, 112:319–329.
Miller RF: D -serine as a glial modulator of nerve cells. Glia 2004, 47:275–283.
Wolosker H, Blackshaw S, Snyder SH: Serine racemase: a glial enzyme synthesizing D -serine to regulate glutamate- N -methyl- D -aspartate neurotransmission. Proc Natl Acad Sci USA 1999, 96:13409–13414.
Molla G, Sacchi S, Bernasconi M, Pilone MS, Fukui K, Polegioni L: Characterization of human D -amino acid oxidase. FEBS Lett 2006, 580:2358–2364.
Henneberger C, Papouin T, Oliet SH, Rusakov DA: Long-term potentiation depends on release of D -serine from astrocytes. Nature 2010, 463:232–236.
Tebano MT, Martire M, Rebola N, Pepponi R, Domenici MR, Gro MC, Schwarzschild MA, Chen JF, Cunha RA, Popoli P: Adenosine A2A receptors and mGluR5 are co-localized and functionally interact in the hippocampus: a possible key mechanism in the modulation of N -methyl- D -aspartate effects. J Neurochem 2005, 95:1188–1200.
Rebola N, Lujan R, Cunha RA, Mulle C: Long-term potentiation of NMDA-EPSCs at hippocampal mossy fiber synapses: an essential role for adenosine A2A receptors. Neuron 2008, 57:121–134.
Ciruela F, Casado V, Rodrigues RJ, Lujan R, Burgueno J, Canals M, Borycz J, Rebola N, Goldberg SR, Mallol J: Presynaptic control of striatal glutamatergic neurotransmission by adenosine A1-A2A receptor heteromers. J Neurosci 2006, 26:2080–2087.
Cunha RA: Adenosine as a neuromodulator and as a homeostatic regulator in the nervous system: different roles, different sources and different receptors. Neurochem Int 2001, 38:107–125.
Mustafa AK, Kim PM, Snyder SH: D -serine as a putative glial neurotransmitter. Neuron Glia Biol 2004, 1:275–281.
Mothet JP, Pollegioni L, Ouanounou G, Martineau M, Fossier P, Baux G: Glutamate receptor activation triggers a calcium-dependent and SNARE protein-dependent release of the gliotransmitter D -serine. Proc Natl Acad Sci USA 2005, 102:5606–5611.
Lawson LJ, Perry VH, Dri P, Gordon S: Heterogeneity in the distribution and morphology of microglia in the normal adult mouse brain. Neuroscience 1990, 39:151–170.
Njie EG, Boelen E, Stassen FR, Steinbusch HW, Borchelt DR, Streit WJ: Ex vivo cultures of microglia from young and aged rodent brain reveal age-related changes in microglial function. Neurobiol Aging 2012, 33:195.e1–12.
Lu WY, Jackson MF, Bai D, Orser BA, MacDonald JF: In CA1 pyramidal neurons of the hippocampus protein kinase C regulates calcium-dependent inactivation of NMDA receptors. J Neurosci 2000, 20:4452–4461.
Rebola N, Simões AP, Canas PM, Tomé AR, Andrade GM, Barry CE, Agostinho PM, Lynch MA, Cunha RA: Adenosine A2A receptors control neuroinflammation and consequent hippocampal neuronal dysfunction. J Neurochem 2011, 117:100–111.
Cristóvão-Ferreira S, Navarro G, Brugarolas M, Pérez-Capote K, Vaz SH, Fattorini G, Conti F, Lluis C, Ribeiro JA, McCormick PJ, Casadó V, Franco R, Sebastião AM: Modulation of GABA transport by adenosine A1R-A2AR heteromers, which are coupled to both Gs- and G(i/o)-proteins. J Neurosci 2011, 31:15629–15639.
Fredholm BB, IJzerman AP, Jacobson KA, Klotz KN, Linden J: International Union of Pharmacology. XXV. Nomenclature and classification of adenosine receptors. Pharmacol Rev 2001, 53:527–552.
Martineau M, Baux G, Mothet JP: D -serine signalling in the brain: friend and foe. Trends Neurosci 2006, 29:481–491.
Vargas Lopes C, Madeira C, Kahn SA, Albino Do Couto I, Bado P, Houzel JC, De Miranda J, De Freitas MS, Ferreira ST, Panizzutti R: Protein kinase C activity regulates D -serine availability in the brain. J Neurochem 2011, 116:281–290.
Fuchs SA, Berger R, de Koning TJ: D -serine: the right or wrong isoform? Brain Res 2011, 1401:104–117.
Rosenberg D, Artoul S, Segal AC, Kolodney G, Radzishevsky I, Dikopoltsev E, Foltyn VN, Inoue R, Mori H, Billard JM, Wolosker H: Neuronal D -serine and glycine release via the Asc-1 transporter regulates NMDA receptor-dependent synaptic activity. J Neurosci 2013. In press
Wolosker H: NMDA receptor regulation by D -serine: new findings and perspectives. Mol Neurobiol 2007, 36:152–164.
Huang YY, Colino A, Selig DK, Malenka RC: The influence of prior synaptic activity on the induction of long-term potentiation. Science 1992, 255:730–733.
Izumi Y, Clifford DB, Zorumski CF: Low concentrations of N -methyl- D -aspartate inhibit the induction of long-term potentiation in rat hippocampal slices. Neurosci Lett 1992, 137:245–248.
Soriano FX, Hardingham GE: Compartmentalized NMDA receptor signalling to survival and death. J Physiol 2007, 584:381–387.
Leveille F, El Gaamouch F, Gouix E, Lecocq M, Lobner D, Nicole O, Buisson A: Neuronal viability is controlled by a functional relation between synaptic and extrasynaptic NMDA receptors. FASEB J 2008, 22:4258–4271.
This work was supported by research funding from: Istituto Pasteur, Fondazione Cenci Bolognetti to CL and PRIN 2009 to CL; MS was supported by the PhD program in Neurophysiology, Sapienza University, Rome. We thank Dr Cristina Marchetti and Dr Davide Ragozzino for critical reading, Dr Bertil B Fredholm for providing us KO mice and critical reading, Francesca Filipponi for helping in mass spectrometry analysis, and Dr Clotilde Lauro and Dr Teresa Ciotti for culture advice.
The authors declare they have no competing interests.
LM, MS and CL conceived and designed the experiments; MS and LM performed and analyzed electrophysiological experiments, MADC participated to patch-clamp experiments; MS and GCh performed stimulation experiments with cultures; LA performed mass spectrometry analysis. GCr provided VT7; LM and CL wrote the paper. All authors have read and approved the final version of the manuscript.