Neuronal MHC Class I Molecules are Involved in Excitatory Synaptic Transmission at the Hippocampal Mossy Fiber Synapses of Marmoset Monkeys
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Several recent studies suggested a role for neuronal major histocompatibility complex class I (MHCI) molecules in certain forms of synaptic plasticity in the hippocampus of rodents. Here, we report for the first time on the expression pattern and functional properties of MHCI molecules in the hippocampus of a nonhuman primate, the common marmoset monkey (Callithrix jacchus). We detected a presynaptic, mossy fiber-specific localization of MHCI proteins within the marmoset hippocampus. MHCI molecules were present in the large, VGlut1-positive, mossy fiber terminals, which provide input to CA3 pyramidal neurons. Furthermore, whole-cell recordings of CA3 pyramidal neurons in acute hippocampal slices of the common marmoset demonstrated that application of antibodies which specifically block MHCI proteins caused a significant decrease in the frequency, and a transient increase in the amplitude, of spontaneous excitatory postsynaptic currents (sEPSCs) in CA3 pyramidal neurons. These findings add to previous studies on neuronal MHCI molecules by describing their expression and localization in the primate hippocampus and by implicating them in plasticity-related processes at the mossy fiber–CA3 synapses. In addition, our results suggest significant interspecies differences in the localization of neuronal MHCI molecules in the hippocampus of mice and marmosets, as well as in their potential function in these species.
KeywordsCalbindin CA3 GFAP Piccolo Neuronal plasticity PSD95 sEPSC VGAT VGlut1 VGlut 2
Cornu ammonis 1
Cornu ammonis 3
Central nervous system
Glial fibrillary acidic protein
Long term depression
Long term potentiation
Miniature excitatory postsynaptic currents
Major histocompatibility complex
Major histocompatibility complex class I
Postsynaptic density protein of 95 kDA
Spontaneous excitatory postsynaptic currents
Vesicular GABA transporter
Vesicular glutamate transporter 1
Vesicular glutamate transporter 2
Major histocompatibility complex class I (MHCI) molecules belong to a large and extremely polymorphic family of cell-surface receptors involved in innate and adaptive immune responses in vertebrates (Solheim 1999). Typical MHCI molecules are heterotrimers composed of a transmembrane heavy chain, a noncovalently attached β-2-microglobulin subunit, and a short peptide comprising 8–15 amino acids that is derived from self or foreign antigens and is presented to cytotoxic T lymphocytes (Solheim 1999; Cresswell et al. 2005). Although virtually all nucleated cells express MHCI molecules, their expression in neurons has remained debatable, as the central nervous system (CNS) is considered immunologically silent (Aarli 1983). However, recent data from rodents demonstrate that MHCI molecules are expressed on the neurons of the CNS and are involved in the modulation of certain plasticity processes in the developing and adult brain (Corriveau et al. 1998; Huh et al. 2000; Goddard et al. 2007; McConnell et al. 2009). MHCI proteins localize to postsynaptic sites in the mouse hippocampus, and hippocampal neurons of MHCI-deficient mice display abnormalities in synapse structure and in basal synaptic transmission (Goddard et al. 2007). MHCI genes are well conserved in mammals; however, there are a number of differences in the organization, structure, and function of these genes between rodents and primates (Kumanovics et al. 2003). Our group has previously demonstrated the expression of certain MHCI genes in the brain of the adult marmoset monkey; their expression patterns in this species appeared comparable to the ones observed in rodents (Rölleke et al. 2006). Here, we describe the expression pattern of a subset of MHCI molecules localized exclusively on the presynaptic side of mossy fiber–CA3 synapses in the marmoset hippocampus. Furthermore, we investigated the properties of excitatory synaptic transmission in acute hippocampal slices of the marmoset monkey and we found that application of antibodies against MHCI interfered with synaptic transmission. The results obtained in this study confirm the emerging role of MHCI molecules in neuronal plasticity and indicate interspecies differences in the expression patterns and functional properties of these proteins in the hippocampus.
Materials and Methods
Fifteen common marmoset monkeys (Callithrix jacchus, 14 males and 1 female) were obtained from the breeding colony at the German Primate Center, Göttingen, Germany. All animal experiments were conducted in accordance with the European Communities Council Directive of November 24, 1986 (86/EEC) and with the National Institutes of Health Guide for the Care and Use of Laboratory Animals, and were approved by the Lower Saxony Federal State Office for Consumer Protection and Food Safety. We investigated healthy, 1 day to 6 years old animals which were also used for other ongoing studies. For expression studies, brain sections were from male animals ranging in age from 1 day old to 6 years old (kindly provided in part by Dr. B. Czéh). Slices for electrophysiology were from 2-, 4-, and 5-year old animals. In all cases, we used the minimum number of animals required to obtain consistent data.
For the detection of MHCI proteins, monoclonal HCA2 and HC10 antibodies were used (Stam et al. 1986, 1990). These antibodies react with polymorphic determinants of classical and some non-classical human MHCI molecules located in the extracellular alpha-1 domain (Stam et al. 1986, 1990; Seitz et al. 1998; Gauster et al. 2007). The antibodies were purified from HCA2 and HC10 hybridoma supernatants (kindly provided by B. Uchanska-Ziegler) via ammonium sulfate precipitation followed by purification using Protein G Sepharose (GE Healthcare, Munich, Germany) according to the manufacturer’s instructions. Antibodies were later dialyzed with Amicon concentrators (Milipore, Billerica, MA, USA) against sterile 0.1 M phosphate-buffered saline (PBS; pH 7.2) and adjusted to concentrations of 2 and 1.5 mg/ml, respectively.
For immunohistochemistry, marmosets were terminally anesthetized with an overdose of ketamine (50 mg/ml), xylazine (10 mg/ml), and atropine (0.1 mg/ml)]. Animals were then perfused transcardially with 0.9% saline, followed by 200 ml of fixative containing 4% paraformaldehyde in 0.1 M sodium phosphate buffer (pH 7.2) for 15 min. The heads were postfixed using the same fixative and the brains were carefully removed from the skulls one day later. After cryoprotection in 0.1 M PBS (pH 7.2) containing 30% sucrose, serial coronal sections (40 μm) were prepared using a cryostat.
Immunocytochemistry for Light Microscopy
Coronal cryosections (40 μm) were collected from marmoset brains containing the hippocampal formation, washed briefly in PBS and quenched of endogenous peroxidase activity by 30 min incubation at room temperature (RT) in 0.5% H202 in distilled water. Sections were rinsed in PBS, blocked for 1 h at RT [3% normal horse serum and 0.03% Triton-X-100 (Sigma) in PBS], incubated 16 h at 4°C with either monoclonal HCA2 IgG (1 mg/ml, 1:500 dilution in 3% normal horse serum and 0.03% Triton-X-100, in PBS) or with control mouse IgG (Sigma), and washed again. Sections were then incubated with biotinylated horse anti-mouse IgG (Vector Laboratories, Burlingame, CA, USA; 1:200 dilution in 3% normal horse serum and 0.03% Triton-X-100, in PBS) for 1 h at RT. After washing, sections were incubated with avidin–biotin–horseradish peroxidase (Vectastain Elite ABC Kit, Vector Laboratories; 1:100 dilution in 3% normal horse serum and 0.03% Triton-X-100, in PBS) for 1 h at RT, washed in PBS and then again in 0.05 M Tris/HCl (pH 7.2) prior to DAB detection (DAB detection with or without nickel enhancement was performed according to the manufacturer’s instructions; DAB-Kit, Vector Laboratories). For immunocytochemistry with HC10 antibody, the epitope retrieval step was perfomed prior to all other steps by incubating the sections for 20 min in 10 mM sodium citrate buffer preheated to 80°C. Sections were later brought to room temperature, washed in PBS and quenched of endogenous peroxidase activity, followed by blocking and incubation in monoclonal HC10 IgG (1 mg/ml, 1:500 dilution in 3% normal horse serum in PBS). All further steps were performed as described above with omission of Triton-X-100 in all the steps. Sections were washed in 0.05 M Tris/HCl (pH 7.6) and again in 0.1 M PBS prior to xylol clearance, dehydration, and coverslipping with Eukitt mounting medium (Kindler, Freiburg, Germany). For Timm’s stain (according to Seress et al. 2001), hippocampal slices (1 mm) were immersed in 0.4% Na2S for 30 min, and then fixed for 16 h in 1% paraformaldehyde and 1.25% glutaraldehyde. The fixed slices were cryoprotected, frozen, and cut into 30-μm sections which were mounted and dried. Sections were then immersed in developer consisting of 30 ml gum Arabic (50%), 5 ml citrate buffer (2 M, pH 3.7), 15 ml hydroquinone (5.67%), and 0.25 ml AgNO3 (17%) for at least 60 min. Digital images of immunostained tissue sections were acquired using the Axiophot II microscope (Zeiss). Final images were assembled in Corel PHOTO-PAINT X3 and are a composition of 4–6 images encompassing the entire hippocampal formation.
Immunofluorescence and Confocal Microscopy
Antibodies used in double-labeling experiments were applied sequentially and blocking steps were performed using normal serum of host species from which respective secondary antibodies were derived. Cryostat sections (40 μm) of marmoset brains containing the hippocampal formation were rinsed in PBS. Non-specific antibody binding sites were blocked with 3% normal serum and 0.03% Triton-X-100 (Sigma) in PBS for 1 h at room temperature. Primary antibodies were used at following dilutions (diluted in 3% normal serum and 0.03% Triton-X-100, in PBS): monoclonal mouse HCA2, 1:500; control mouse IgG 1:500 (Sigma); rabbit anti-PSD95 (Cell Signaling Technology, Danvers, MA, USA), 1:200; rabbit anti-Piccolo, 1:200; rabbit anti-VGlut1, 1:1,000; rabbit anti-VGlut2, 1:200; rabbit anti VGAT, 1:200; rabbit anti-GFAP, 1:200 (all from Synaptic Systems, Göttingen, Germany); rabbit anti-calbindin, 1:200 and sheep anti-TH, 1:200 (both from Chemicon International Ltd., Hampshire, UK). Secondary antibodies (Alexa 488-coupled donkey anti mouse, Alexa 568-coupled goat anti-rabbit and Alexa 594-coupled donkey anti-sheep, Molecular Probes, Invitrogen, Leiden, Netherlands) were used at 1:500 dilution (diluted in 3% normal serum and 0.03% Triton-X-100, in PBS). After the antibody incubation steps, sections were washed in PBS and floated/mounted on Histobond slides in distilled water, allowed to dry overnight at 4°C and coverslipped with mounting medium (Aqua-Polymount, Polysciences Inc., Warrington, PA, USA).
Confocal microscopy was performed using a laser-scanning microscope (LSM 5 PASCAL, Zeiss) with argon (488 nm) and helium/neon (543 nm) lasers. Confocal analysis was performed in multiple-tracking mode to avoid bleed through between channels. High magnification images were obtained as z-series stacks of a region containing mossy fiber terminals at a resolution of 2,048 × 2,048 using an Apochromat 63 × oil objective (NA = 1.4) and immersion oil (Immersol, Zeiss; refractive index = 1.518). The 543 nm laser was always used with a smaller detection pinhole diameter than the 488 nm laser to produce optical sections of comparable thickness for colocalization analysis. For substantia nigra, images were taken from single plane at a resolution of 1,024 × 1,024 using an Apochromat 63 × oil objective (NA = 1.4) and immersion oil (Immersol, Zeiss; refractive index = 1.518). For quantification of colocalization signals, intensity correlation coefficients (ICQ, Li et al. 2004) were obtained using the ImageJ colocalization plug-in (Abramoff et al. 2004) for a minimum of three images per animal. These values were compared between the two groups using the Student’s t-test (GraphPad Prism version 4 for Windows, San Diego, CA, USA). The region of interest (ROI) was defined using the green channel (MHCI signal).
PCR Cloning of MHC Class I Transcripts
Isolation of the common marmoset MHC class I cDNA sequence was carried out by reverse transcriptase polymerase chain reaction (RT-PCR). 1 μg of total brain RNA was reverse transcribed using oligo-d(T) primer (GACTCGAGTCGACATCGA(T)17) and 400 U of reverse transcriptase (Promega, Mannheim, Germany). An aliquot of this reaction was used as template in a PCR containing the primers. The primers were designed using Primer3 program (Rozen and Skaletsky 2000) and were intended to amplify full length marmoset MHC class I transcripts. Primer sequences were carrying BamHI restriction sites and were as follows: forward 5′-CACGGATCCCACTTTACAAGCCGTGAGAGAC-3′, reverse 5′-CACGGATCCCTCCTGTTGCTCTCGGGGGCCTTG-3′. Caja-G*1 (Accesion number: U59637) was obtained and cloned in pEXPR-IBA103 (IBA Technologies, Göttingen, Germany).
Protein Extraction and Immunoblot Analysis
Brains were immediately removed from terminally anesthetized animals [by an overdose of ketamine (50 mg/ml), xylazine (10 mg/ml), and atropine (0.1 mg/ml)]. Hippocampi were quickly dissected and homogenized using a Dounce homogenizer (tight pestle) in ice-cold homogenization buffer consisting of 50 mM Tris/HCl (pH 7.4), 7.5% glycerol, 150 mM NaCl, 1 mM EDTA, 1% Triton X-100, and complete protease inhibitor cocktail tablets (Roche Diagnostics, Mannheim, Germany). After homogenization, samples were centrifuged at 4,000 × g for 20 min at 4°C. The resulting supernatants were centrifuged again until they were clear. Protein concentration was measured using the Bio-Rad DC Protein assay (Bio-Rad Laboratories, Hercules, CA, USA). Protein preparations were electrophoresed in 12.5% SDS gels under reducing conditions. Proteins were subsequently transferred to nitrocellulose (Schleicher and Schuell, Dassel, Germany) by semi-dry electroblotting for 2 h at 1 mA/cm2 in transfer buffer containing 25 mM Tris base, 150 mM glycine, and 10% (v/v) methanol. After transfer, the blot was blocked with 5% (w/v) milk powder and 0.1% Tween-20 in PBS for 1 h at room temperature, and then incubated with monoclonal HCA2 (1:1000) or monoclonal HC10 (1:1000) antibodies or control mouse IgG (Sigma) overnight at 4°C. After washing three times for 5 min in PBS/0.1% Tween, the blot was incubated for 1 h at room temperature with horseradish peroxidase coupled goat anti-mouse IgG (1:4000, Santa Cruz Biotechnology, Santa Cruz, CA, USA). Prior to visualization, the blot was washed in PBS/0.1% Tween (3 × 5 min) and once more in PBS. Signals were visualized by SuperSignal West Dura enhanced luminescence substrate (Pierce Biotechnology, Rockford, IL, USA).
Cell Culture and Immunoprecipitation
HEK293T cells were transfected with linearized, full-length Caja-G carrying a C-terminal One-STrEP-tag in pEXPR-IBA103 (IBA Technologies) using Fugene 6 (Roche, Indianapolis, IN, USA) as described by the manufacturer. Stable clones were selected with Geniticine (G418, Life Technologies, Karlsruhe, Germany) and further propagated. Protein extracts were obtained as described above. Purified Caja-G carrying a C-terminal One-STrEP-tag was obtained following manufacturer’s protocol (IBA Technologies). For immunoprecipitation, 1 mg/ml of protein extract was precleared with Protein G Sepharose Fast Flow (GE Healthcare) for 1 h at 4°C. Samples were centrifuged briefly and supernatant was incubated with either monoclonal HCA2 IgG (5 μg) or monoclonal HC10 IgG (5 μg) or without antibodies overnight on rotary platform at 4°C, after which they were incubated with Protein G Sepharose Fast Flow (GE Healthcare) for 1 h at 4°C. Samples were then centrifuged and pellets were washed three times with lysis buffer [50 mM Tris/HCl pH 7.4, 150 mM NaCl, 1 mM EDTA, 1% Triton-X 100 and complete protease inhibitor cocktail tablet (Roche Diagnostics, Mannheim, Germany)]. The bound proteins were eluted by boiling in Laemmli buffer and western blot was performed as described above. After transfer, the blot was blocked with 5% (w/v) BSA (Sigma) and 0.1% Tween-20 in PBS for 1 h at room temperature, and then incubated with monoclonal anti-STrEP HRP-conjugated antibody (1:4000 dilution, IBA Technologies) overnight at 4°C according to the manufacturer’s instructions. After washing three times for 5 min in PBS/0.1% Tween and once more in PBS, signals were visualized by SuperSignal West Pico enhanced luminescence substrate (Pierce Biotechnology).
Animals were terminally anesthetized with an overdose of ketamine (50 mg/ml), xylazine (10 mg/ml), and atropine (0.1 mg/ml) and intracardially perfused with ice-cold oxygenated (95% O2 and 5% CO2) modified artificial cerebrospinal fluid (ACSF) containing (in mM): sucrose 220; KCl 1.9; Na2HPO4 1.25; glucose 10; NaHCO3 33; MgCl2 26; CaCl2 20.5; kynurenic acid 2; and ascorbic acid 2 (all from Sigma). Transverse hippocampal slices (300–400 μm) were prepared using a vibroslicer (752 M, Campden Instruments, Loughborough, UK), transferred to the recording chamber, and allowed to recover at 33°C for at least 90 min, after which they were kept at room temperature. Recordings were performed on slices placed in a submerged chamber perfused with oxygenated ACSF (33°C) containing (in mM): NaCl 124; KCl 5; Na2HPO4 1.25; glucose 10; NaHCO3 26; MgSO4 2; CaCl2 2; and ascorbic acid 1 (all from Sigma). The recording chamber was continuously perfused with ACSF and aerated with 95% O2 and 5% CO2 (2–3 ml/min). The temperature was kept at 33°C. CA3 neurons were visually identified using infrared microscopy. The pipette solution contained (in mM): potassium gluconate 135; MgCl2 2; CaCl2 0.1; EGTA 1; Na2 ATP 2; Na2 GTP 0.5; and HEPES 10. Spontaneous glutamatergic excitatory postsynaptic currents (sEPSCs) were recorded in the presence of 1 μM strychnine and 1 μM bicuculline, as described by Medrihan et al. (2008). Either control IgG or a mixture of HCA2 and HC10 antibodies at a concentration of 1.5 mg/ml each were directly applied in close proximity to neurons using glass pipettes (a schematic representation of the recording chamber set-up is provided in Supplementary figure 3). The tip size of the pipette, pressure (0.5 mbar), and application time (0.5 s) were kept constant in all experiments. In addition, the distance between the pipette tip and the cells was monitored using a camera with a liquid–crystal display device and was kept constant in all experiments. Recordings of selected cells were first performed for 3 min without antibody application (control recording); the antibodies were then applied for 20 min at 30 s intervals. Patches with a serial resistance of >10 MΩa, membrane resistance of <0.2 GΩ, or leak currents of >200 pA were excluded. The membrane currents were filtered by a four-pole Bessel filter at a corner frequency of 2 kHz and digitized at a sampling rate of 5 kHz using the DigiData 1322A interface (Molecular Devices, Sunnyvale, CA, USA). Data acquisition and analysis were done using commercially available software: pClamp 9.0 (Molecular Devices), MiniAnalysis (SynaptoSoft, Decatur, GA, USA) and Prism 4 for Windows (GraphPad Software).
MHCI Proteins Localize to Mossy Fibers in the Common Marmoset Hippocampus
The anatomy of the primate hippocampus is well characterized (Seress 2007) and a number of studies on MHCI in mice have been performed in this brain region (Corriveau et al. 1998; Huh et al. 2000; Goddard et al. 2007). Therefore, we decided to focus on MHCI in the hippocampal mossy fibers in order to draw potential parallels between different findings in this and other studies more easily.
Glial fibrillary acidic protein (GFAP) is a well established marker of brain astrocytes (Eng et al. 2000). Double labeling experiments revealed only occasional colocalizations of GFAP and MHCI signals (Fig. 2e–h). High magnification images revealed MHCI signals dispersed between GFAP-positive astrocyte processes (Fig. 2h, white arrows).
MHCI Proteins are Mainly Present in the Giant Mossy Fiber Terminals
Neuronal MHCI Proteins are Involved in Excitatory Transmission at Mossy Fiber–CA3 Synapses in the Marmoset Hippocampus
Expression of MHC class I molecules in neurons of the CNS has been debated over the years. The dogma of the immune privilege of the brain supports the notion that neurons normally do not express MHCI proteins, and that neuronal MHCI molecules can only be observed after induction by cytokines (Neumann et al. 1995). However, several recent studies performed in rodents provide experimental evidence emphasizing an important role for MHCI molecules in the modulation of synaptic plasticity and in the proper development of brain circuitry in the normal, noninjured brain (Corriveau et al. 1998; Huh et al. 2000; Goddard et al. 2007).
Although there are some differences in the structure and function of molecules in the MHCI family between rodents and primates, previous results reported by our group suggested a relatively conserved expression pattern of a subset of MHCI molecules in the brains of rodents and nonhuman primates (Rölleke et al. 2006). MHCI molecules are very numerous and are usually divided into classical and non-classical MHCI molecules. Classical MHCI molecules are in general associated with immune responses, while the non-classical MHCIs have more elusive roles, especially outside of the immune system (Arosa et al. 2007). In rodents, classical MHCI genes have recently been implicated in synaptic refinement and the maintenance of synaptic plasticity in cerebellum and visual system (Datwani et al. 2009; McConnell et al. 2009). The non-classical MHCI subset is believed to be involved in the proper development of the vomeronasal organ in mice (Ishii and Mombaerts 2008). We believe that the subset previously detected by us in the marmoset brain belongs to the non-classical MHCI molecules (Rölleke et al. 2006). In this study, however, another subset of MHCI proteins displayed distinct and so far unreported expression patterns and properties.
Staining with antibodies that target the heavy-chain subunit of the classical MHCI molecules revealed a strong MHCI expression confined to the mossy fibers in the hippocampal formation. Both antibodies used here targeted an epitope situated in the most polymorphic region of the MHCI molecules; therefore, these antibodies are specific for only a small portion of MHCI proteins. In humans, these antibodies recognize the classical MHCI molecules and (in case of the HCA2 antibody) some non-classical MHCI (Stam et al. 1986, 1990; Seitz et al. 1998; Gauster et al. 2007). The marmoset MHCI genes are yet to be characterized, but based on what has previously been published on this topic (Cadavid et al. 1997) and on the data available for the epitopes of these antibodies (Stam et al. 1986, 1990; Seitz et al. 1998; Gauster et al. 2007), we believe that the MHCI detected in this study belongs to the classical subset. Both antibodies recognized bands of the appropriate size on western blots and, with respect to the neuronal staining, yielded almost identical staining patterns in immunocytochemical experiments, which supports their specificity. In addition, both HCA2 and HC10 immunoprecipitated a native, classical marmoset MHCI protein, Caja-G.
Our double-labeling experiments suggest that MHCI proteins are localized on the nerve terminals, and not on glial processes. Furthermore, our experiments suggest that the MHCI proteins targeted here are presynaptic and primarily associated with the large mossy fiber boutons, which provide the main excitatory input to CA3 pyramidal neurons. Thus, the present results from marmosets differ from previous findings in mice, in which a postsynaptic role of MHCI proteins was discussed (Goddard et al. 2007). In accordance with the presynaptic localization detected here, MHCI proteins have recently been reported in the nerve terminals at the neuromuscular junction in mice (Thams et al. 2009). The fact that no MHCI proteins were detected in the hippocampal mossy fibers of mice may be due to a lack of suitable antibodies against mouse MHCI proteins. However, it is also possible that MHCI expression in mossy fibers is a marmoset (or primate)-specific trait. As previously mentioned, the non-classical MHCI molecules exhibit expression patterns that are very similar to the one detected in rodents (Corriveau et al. 1998; Rölleke et al. 2006). Given the high evolution rate of MHCI molecules (Kumanovics et al. 2003), it is likely that a fraction of classical MHCI proteins developed a new function and localization. A detailed comparative study between rodents and primates using equivalent tools is needed to elucidate this issue. However, the results obtained using whole-cell patch-clamp recordings in marmoset CA3 neurons suggest the presence of interspecies differences.
Electrophysiology in nonhuman primates is not commonly employed given that mouse models are usually readily available. Furthermore, ethical standards regarding the use of nonhuman primates in neurobiological research limit the number of primates as experimental animals, and the preparation of acute brain slices from primates is more arduous compared to the preparation of rodent acute brain slices. However, the opposing results with respect to the localization of MHCI molecules in the hippocampus of mice and marmosets did not allow us to use mice for electrophysiological experiments. In addition, we felt it was important to elucidate the function of neuronal MHCI in the primate hippocampus precisely because of the pronounced interspecies differences in their localization within the hippocampal formation. As MHCI knockout marmosets or specific neuronal MHCI antagonists are not currently available, we used antibodies to block MHCI on the surface of mossy fiber terminals. The effects observed were not an artifact of the antibody application, as there was no significant effect of the application of control immunoglobulins in the same concentration (Fig. 6). Previously published data suggest that the use of antibodies that block cell-surface receptors is an adequate method for investigating the function of proteins for which knockout models or antagonists are not available (Bufler et al. 1996; Saghatelyan et al. 2000; Mameli et al. 2005).
In our experiments, the normalized mean frequency of sEPSCs was significantly reduced after application of the blocking antibodies and this effect increased proportionally with the duration of the incubation. Furthermore, we observed a small, but significant transient increase in the amplitude of sEPSCs (Fig. 6). These results did not match previous observations in rodents where it has been found that the lack of surface MHCI expression leads to an increase in mEPSCs (miniature EPSCs) frequency of hippocampal neurons (Goddard et al. 2007). As already mentioned, it is possible that the MHCI molecules targeted in the present study belong to a subset of MHCIs that has not yet been detected in mice because of the unavailability of proper antibodies. However, the mice used in the previous studies lacked expression of the majority of, if not all, MHCI genes (Goddard et al. 2007). On the other hand, we recorded sEPSCs here, not mEPSCs (as in the study in mice), which may also account for some of the differences observed.
It is obvious that evolution provided MHCI molecules with a number of diverse functions, both immune and nonimmune (Fishman et al. 2004). A potential explanation for the function of MHCI at the mossy fiber–CA3 synapses arises when previous studies on MHCI are taken into consideration. The mossy fiber–CA3 synapse displays a number of peculiarities when compared with the majority of CNS synapses. For instance, it is characterized by a low basal neurotransmission, which is maintained via the activation of receptors that have inhibitory effects on synaptic transmission (Nicoll and Schmitz 2005). Given that the best characterized nonimmune function of MHCI molecules is the regulation of trafficking and internalization of various receptors (Arosa et al. 2007), we hypothesize that the function of neuronal MHCI proteins (consistent with the results obtained here) is the proper internalization of one or several of those receptors. One may speculate that blocking the interaction of MHCI molecules with their receptors by application of anti-MHCI antibodies would prolong inhibitory signaling, thus reducing the frequency of sEPSCs. This does not fully explain the transient increase in the amplitude of sEPSCs: although changes in the amplitude of the spontaneous currents usually imply a defect in the postsynapse, sometimes they may also be a reflection of a presynaptic mechanism (Sharma and Viijayaraghavan 2003). Further electrophysiological analyses are required to dissect the action of MHCI proteins in synaptic transmission. The identification of interacting partner(s) and signaling mechanisms are crucial to the elucidation of the function of neuronal MHCI molecules.
In conclusion, the present study contributes to the growing body of evidence that MHCI molecules are involved in synaptic plasticity processes in the CNS. It remains unclear whether the presynaptic and mossy fiber-specific expression of MHCI molecules observed in this study is marmoset specific, or whether it is a characteristic of all nonhuman primates. A number of proteins display differential localization in rodents and primates, which is usually taken as a possible basis for the evolution of the primate brain with respect to cognitive functions. Furthermore, a concept of MHCI signaling in neurons has very important implications, particularly when considering autoimmune diseases that affect the CNS and various diseases genetically linked to the MHC, such as autism (Belmonte et al. 2004). With this in mind, further research is required to elucidate the exact mechanisms of the action of nonhuman primate neuronal MHCI, particularly regarding interspecies expression differences.
The authors wish to thank T. Meyer-Burhenne and S. Leineweber for expert animal care, A. Hoffmann, J. Krenzek, S. Kosin, A. Heutz, and A. Zank for technical assistance, Dr. B. Czéh for assistance with the Timm’s staining protocol, Dr. L. Medrihan for help establishing the patch clamp recording techniques and Dr. B. Cooper for invaluable advice regarding synaptic markers. AR was supported by an EC fellowship for Neuroscience Early Stage Research Training (NEUREST) and was a student of the MSc/PhD Molecular Biology Graduate Program in Göttingen, Germany. This work was supported by EU grant NEST-28594 and the SFB 449, TP B6.
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