Dopamine-galanin receptor heteromers modulate cholinergic neurotransmission in the rat ventral hippocampus

Abstract

Previous studies have shown that dopamine and galanin modulate cholinergic transmission in the hippocampus, but little is known about the mechanisms involved and their possible interactions. By using resonance energy transfer techniques in transfected mammalian cells we demonstrated the existence of heteromers between the dopamine D₁-like receptors (D₁ and D₅) and galanin Gal_1, but not Gal₂ receptors. Within the D₁-Gal₁ and D₅-Gal₁ receptor heteromers, dopamine receptor activation potentiated and dopamine receptor blockade counteracted MAPK activation induced by stimulation of Gal₁ receptors, while Gal₁ receptor activation or blockade did not modify D₁-like receptor-mediated MAPK activation. Ability of a D₁-like receptor antagonist to block galanin-induced MAPK activation (cross-antagonism) was used as a “biochemical fingerprint” of D₁-like-Gal₁ receptor heteromers, allowing their identification in the rat ventral hippocampus. The functional role of D₁-like-Gal receptor heteromers was demonstrated in synaptosomes from rat ventral hippocampus, where galanin facilitated acetylcholine release, but only with co-stimulation of D₁-like receptors. Electrophysiological experiments in rat ventral hippocampal slices showed that these receptor interactions modulate hippocampal synaptic transmission. Thus, a D₁-like receptor agonist, that was ineffective when administered alone, turned an inhibitory effect of galanin into an excitatory effect, an interaction that required cholinergic neurotransmission. Altogether, our results strongly suggest that D₁-like-Gal₁ receptor heteromers act as processors that integrate signals of two different neurotransmitters, dopamine and acetylcholine, to modulate hippocampal cholinergic neurotransmission.

The neuropeptide galanin is widely distributed in the central nervous system (Melander et al., 1986a,b; Hökfelt et al., 1998; Ögren et al., 1998), where it is co-released with noradrenaline, serotonin, histamine and acetylcholine (ACh) (Hökfelt et al., 1998). Particular attention has been given to the presence of galanin in a population of cholinergic neurons in the septal nucleus and diagonal band of Broca, which project to the hippocampal formation (Melander et al., 1985), because of its possible relevance for learning, memory and Alzheimer’s disease (Ögren et al., 1998; Mitsukawa et al., 2008). Gal₁ and Gal₂ receptors are the predominant galanin receptor subtypes in the brain and, together with the less populated subtype Gal₃, they belong to the G-protein-coupled receptor (GPCR) family (Branchek et al., 2000). The lack of selective ligands and reliable antibodies (Hawes and Picciotto, 2005) has made it difficult to identify the distribution of Gal₁ and Gal₂ receptors in the septo-hippocampal system. Gal₁ mRNA is highly expressed in the septal area, where Gal₂ mRNA expression is moderate and confined to a few scattered neurons (Parker et al., 1995; O’Donnell et al., 1999). ¹²⁵I-galanin binding sites in the ventral hippocampus are significantly reduced following lesions of the septo-hippocampal projection, which eliminates most cholinergic input to the ventral hippocampus (Fisone et al., 1987). This provided clear evidence for the existence of a significant population of presynaptic hippocampal galanin receptors localized in cholinergic nerve terminals, although the galanin receptor subtype involved is still a matter of debate (Miller et al, 1997). With postsynaptic galanin receptors, Gal₁ is preferentially expressed in the ventral hippocampus, CA1 and subiculum, while Gal₂ is expressed in the dentate gyrus of both ventral and dorsal hippocampus (O’Donnell et al., 1999).

In vivo studies in rodents with central administration of galanin have suggested that galanin inhibits cholinergic neurotransmission in the ventral hippocampus (Fisone et al., 1987; Ögren et al., 1998; Laplante et al., 2004a). Furthermore, central administration of galanin leads to cognitive deficits in a variety of tasks (Crawley, 1996; Ögren et al., 1998). However, recent post-mortem studies on brains from Alzheimer's disease patients suggest that galanin may instead stimulate cholinergic neurotransmission, which could attenuate the development of Alzheimer's symptoms (Counts et al., 2008; Ögren et al., 2010).

In addition to galanin, dopamine also plays a key modulatory role in the septo-hippocampal cholinergic pathway. Initial studies showed that dopamine facilitates hippocampal ACh release by acting on D₁-like receptors, that are thought to be located in hippoccampal cholinergic terminals (Hersi et al., 1995). Of the two D₁-like receptor subtypes, D₁ and D₅, the D₅ is the predominant subtype in the hippocampus (Ciliax et al., 2000) and, the one most probably involved in the modulation of hippocampal ACh release (Hersi et al., 2000; Laplante et al., 2004b). In the present study we demonstrate that dopamine and galanin work in concert to modulate cholinergic neurotransmission in the ventral hippocampus and that this modulation can occur via heteromers between D₁ or D₅ receptors and Gal₁ receptors.

Materials and Methods

Animals

Male Wistar rats (4–7 weeks old), from Harlan Interfauna Iberica, SL (Barcelona), were housed in a temperature (21 ± 1°C) and humidity-controlled (55 ± 10%) room with a 12:12 hours light/dark cycle with food and water ad libitum. Animal procedures were conducted according to standard ethical guidelines (European Communities Council Directive 86/609/EEC) and approved by the local (Portuguese or Spanish) ethical committees. Rats were anesthetized with isoflurane before decapitation.

Cell culture

Human embryonic kidney (HEK-293T) cells were grown in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 2 mM L-glutamine, 100 µg.ml⁻¹ sodium pyruvate, 100 units/ml penicillin/streptomycin, and 5% (v/v) heat inactivated Fetal Bovine Serum (FBS) (all supplements were from Invitrogen, Paisley, Scotland, UK). Chinese hamster ovary (CHO) cells were cultured in MEM alpha medium without nucleosides supplemented with 100 units/ml of penicillin/streptomycin and 10% (v/v) heat-inactivated Fetal Bovine Serum (FBS). HEK-293T and CHO cells were maintained at 37°C in a humidified atmosphere of 5% CO₂, and were passaged when they were 80–90% confluent, i.e. approximately twice a week.

Fusion proteins and expression vectors

The cDNAs for D₁, D₅, Gal_1, Gal_2, cannabinoid CB₁ and serotonin 5HT_2B receptors cloned into pcDNA3.1 were amplified without their stop codons using sense and antisense primers harboring unique EcoRI and BamHI sites to clone D₁, D₅ and 5HT_2B receptors and EcoRV and KpnI sites to clone Gal₂ receptors in Rluc vector or EcoRI and BamHI to clone D₁, D₅ and CB₁ receptors and EcoRI and KpnI to clone Gal₁ receptor in EYFP vector. The amplified fragments were subcloned to be in-frame into restriction sites of pcDNA3.1-Rluc (Renilla luciferase; Clontech, Heidelberg, Germany) or pEYFP-N1 (enhanced yellow variant of GFP; Clontech) vectors resulting in the plasmids D₁-Rluc, D₁-YFP, D₅-Rluc, D₅-YFP, Gal₁-YFP and Gal₂-Rluc. Expression of constructs was tested by confocal microscopy and the receptor functionality by second messengers, ERK1/2 phosphorylation (see results). The cDNA encoding the C terminus of the rat D₁ or D₅ receptors (D1CT and D5CT, respectively) were amplified from Rat Brain QUICK-Clone cDNA (Clontech) by PCR using following primers: D1-CT1012F (CAG AAG GCG TTC TCA ACC) and D1-CT1321R (AGT GGA ATG CTG TCC ACT) or D₅-CT1051F (CCC ATC ATC TAT GCC TTT AAT GCA GAC TTC) and D₅-CT1425R (AGC AGT TTT ATC GAA ACA ATT GGG GGT GAG). The cDNA encoding D₁CT or D₅CT were subcloned into the BamHI/EcoRI sites of pGEX-4T-1 (Amersham Biosciences). A GST fusion proteins containing the C terminus of the rat D₁ or D₅ receptors (GST-D₁CT and GST-D₅CT respectively) were generated corresponding to amino acid residues 227–335 of the rat D₁ receptor and amino acid residues 358–475 of the rat D₅ receptor. Bacterial BL21 (DE3) cells with pGEX-4T-1/Drd5CT plasmid were grown overnight in imMedia™ medium (Invitrogen) using ampicillin selection. Protein production was induced with 0.5 mM isopropyl-β-d-thiogalactopyranoside (Sigma) at 20° C for 18 h. Bacteria were harvested by centrifugation at 7,500 g for 15 min at 4°C, and the pellet was suspended in cold PBS buffer with 1 mM PMSF and a protease inhibitor mixture (Roche). Cells were lysed by sonication and the lysate was incubated for 1 hour with 1% triton 100 and centrifuged at 18,000 × g for 10 min at 4°C. The supernatant was collected for purification of GST fusion protein. Purification of fusion proteins was performed using Glutathione 4B Sepharose™ bead matrix (GE Healthcare) as described by manufacturer.

Transient transfection and protein determination

HEK-293T or CHO cells growing in 35-mm diameter wells of 6-well plates were transiently transfected with the corresponding fusion protein cDNA by the ramified PEI (PolyEthylenImine, Sigma, St. Louis, MO, USA) method. Cells were incubated (4 h) with the corresponding cDNA together with ramified PEI (5 ml/mg cDNA of 10 mM PEI) and 150 mM NaCl in a serum-starved medium. After 4 hours, the medium was changed to a fresh complete culture medium. Forty-eight hours after transfection, cells were washed twice in quick succession in Hanks' balanced salt solution HBSS (137 mM NaCl, 5 mM KCl, 0.34 mM Na2HPO4×12H2O, 0.44 mM KH2PO4, 1.26 mM CaCl2×2H2O, 0.4 mM MgSO4×7H2O, 0.5 mM MgCl2, 10 mM HEPES, pH 7.4) supplemented with 0.1% glucose (w/v), detached by gently pipetting and resuspended in the same buffer. To control the cell number, sample protein concentration was determined using a Bradford assay kit (Bio-Rad, Munich, Germany) using bovine serum albumin dilutions as standards. HEK-293T cells suspension (20 µg of protein) was distributed into 96-well microplates; black plates with a transparent bottom (Porvair, King’s Lynn, UK) were used for fluorescence determinations, while white opaque plates (Sigma) were used for BRET experiments

BRET assays

HEK-293T cells were transiently co-transfected with the indicated amounts of plasmid cDNAs corresponding to the indicated fusion proteins (see figure legends). To quantify fluorescence proteins, cells (20 µg protein) were distributed in 96-well microplates (black plates with a transparent bottom) and fluorescence was read in a Fluo Star Optima Fluorimeter (BMG Labtechnologies, Offenburg, Germany) equipped with a high-energy xenon flash lamp, using a 10 nm bandwidth excitation filter at 400 nm reading. Receptor-fluorescence expression was determined as fluorescence of the sample minus the fluorescence of cells expressing protein-Rluc alone. For BRET measurements, the equivalent of 20 µg of cell suspension were distributed in 96-well microplates (Corning 3600, white plates; Sigma) and 5 µM coelenterazine H (Molecular Probes, Eugene, OR) was added. After 1 minute of adding coelenterazine H, readings were collected using a Mithras LB 940 (Berthold, Bad Wildbad, Germany) that allows the integration of the signals detected in the short-wavelength filter at 485 nm (440–500 nm) and the long-wavelength filter at 530 nm (510–590 nm). To quantify receptor-Rluc expression, luminescence readings were performed after 10 minutes of adding 5 µM coelenterazine H. Cells expressing BRET donors alone were used to determine background. The net BRET is defined as [(long-wavelength emission)/(short-wavelength emission)]-Cf where Cf corresponds to [(long-wavelength emission)/(short-wavelength emission)] for the Rluc construct expressed alone in the same experiment. Curves were fitted using a non-linear regression equation and assuming a single phase (GraphPad Prism software, San Diego, CA, USA).

Immunocytochemistry

After 48 h of transfection, HEK-292T cells were fixed in 4% paraformaldehyde for 15 min and washed with phosphate-buffered saline (PBS) containing 20 mM glycine (buffer A) to quench the aldehyde groups. Cells were permeabilized with buffer A containing 0.05% Triton X-100 for 5 min and then were treated with PBS containing 1% bovine serum albumin. After 1 h at room temperature, protein-Rluc was labelled with the primary mouse monoclonal anti-Rluc antibody (1/100, Chemicon, Billerica, MA) for 1 h, washed and stained with the secondary antibody Cy3 Donkey anti-mouse (1/200, Jackson Immunoresearch Laboratories, West Grove, PA, USA). Protein-YFP was detected by its fluorescence properties. The slides were rinsed several times and mounted with a medium suitable for immunofluorescence (30% Mowiol, Calbiochem, Darmstadt, Germany). The samples were observed in a Leica SP2 confocal microscope (Leica Microsystems, Mannheim, Germany).

Pull-down assay

HEK293 cells were collected after 48 hours of transfection with 25 µg Gal₁-YFP, Gal₂-YFP or pEYFP-N1 plasmid (control) and extracted in cell extraction buffer (10 mM Tris, pH 7.4, 100 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1 mM NaF, 20 mM Na4P2O7, 2 mM Na3VO4, 1% Triton X-100, 10% glycerol, 0.1% SDS, 0.5% deoxycholate) with 1 mM PMSF and a the protease inhibitor mixture (Roche) for 30 minutes on ice. The cell extracts were centrifuged at 16,000 g for 10 min at 4°C and the supernatant was used for pull-down experiments. Pull-down experiments were performed by incubating cell extracts (135 RFUs/800 µl) with 50 µg GST-D₁CT, GST-D₅CT or GST for two hours with constant rotation at 4°C. Then, 30 µl Glutathione 4B Sepharose™ beads were added and incubation was prolonged for 1 hour. The beads were then washed four times with cold wash buffer (TBS, 0.1% Triton X-100, and protease inhibitor mixture). Subsequently, 50 µl of elution buffer (10 mM reduced glutathione in 50 mM Tris-HCl pH 8.0) were added to each sample and kept for 10 min at room temperature. Fluorescence in the eluted solution was measured with SpectraMax® M5 Microplate Readers (Molecular Devices) using 514 nm wavelength excitation and 596 nm wavelength emission filters. Differences in relative fluorescence units among the different groups were statistically analyzed with repeated measures ANOVA with Bonferroni’s correction.

ERK phosphorylation assay

Transfected CHO cells were cultured in serum-free medium for 16 h before the addition of any agent. For assays in hippocampal slices, rat brains were rapidly removed and placed in ice-cold oxygenated (O₂/CO₂: 95%/5%) Krebs-HCO₃⁻buffer (124 mM NaCl, 4 mM KCl, 1.25 mM NaH₂PO₄, 1.5 mM MgCl₂, 1.5 mM CaCl₂, 10 mM glucose and 26 mM NaHCO₃, pH 7.4). The brains were sliced perpendicularly to the long axis of the hippocampus at 4°C. Slices (400-µm-thick) were kept at 4°C in Krebs-HCO₃⁻buffer during the dissection. Each hippocampal slice was transferred into an incubation tube containing 1 ml of ice-cold Krebs-HCO₃⁻ buffer (124 mM NaCl, 4 mM KCl, 1.25 mM NaH₂PO₄, 1.5 mM MgCl₂, 1.5 mM CaCl₂, 10 mM glucose and 26 mM NaHCO₃,. The temperature was raised to 23°C and after 30 min, the media was replaced by 2 ml of fresh Krebs-HCO₃⁻ buffer (23°C) with similar composition. The slices were incubated under constant oxygenation (O₂/CO₂: 95%/5%) at 30°C for 4–5 h in an Eppendorf Thermomixer (5 Prime, Inc., Boulder, CO, USA). The media was replaced by 200 µl of fresh Krebs-HCO₃⁻ buffer and incubated for 30 min before the addition of any agent. Cells or slices were treated or not with the indicated ligand for the indicated time and were rinsed with ice-cold phosphate-buffered saline and lysed by the addition of 500 µl of ice-cold lysis buffer (50 mM Tris-HCl pH 7.4, 50 mM NaF, 150 mM NaCl, 45 mM β-glycerophosphate, 1% Triton X-100, 20 µM phenyl-arsine oxide, 0.4 mM NaVO₄ and protease inhibitor cocktail). The cellular debris was removed by centrifugation at 13,000xg for 5 min at 4°C and the protein was quantified by the bicinchoninic acid method using bovine serum albumin dilutions as standard. To determine the level of ERK1/2 phosphorylation, equivalent amounts of protein (10 µg) were separated by electrophoresis on a denaturing 7.5% SDS-polyacrylamide gel and transferred onto PVDF-FL membranes. Odyssey blocking buffer (LI-COR Biosciences, Lincoln, Nebraska, USA) was then added and the membrane was rocked for 90 min. The membranes were then probed with a mixture of a mouse anti-phospho-ERK1/2 antibody (1:2500, Sigma) and rabbit anti-ERK1/2 antibody that recognizes both, phosphorylated and non-phosphorylated ERK1/2 (1:40000, Sigma) for 2–3 h. Bands were visualized by the addition of a mixture of IRDye 800 (anti-mouse) antibody (1:10000, Sigma) and IRDye 680 (anti-rabbit) antibody (1:10000, Sigma) for 1 h and scanned by the Odyssey infrared scanner (LI-COR Biosciences, Lincoln, Nebraska, USA). Bands densities were quantified using the scanner software, exported to Excel (Microsoft, Redmond, WA, U.S.A). The level of phosphorylated ERK1/2 isoforms was normalized for differences in loading using the total ERK protein band intensities. Statistical differences between the different groups were analyzed by one-way ANOVA with Bonferroni’s correction.

[³H]Ach release from hippocampal synaptosomes

The synaptosomal fraction was prepared as routinely (see e.g. Vaz et al., 2008). Briefly, after decapitation under halothane anesthesia, the brains were rapidly removed into ice-cold continuously oxygenated (O₂/CO₂: 95%/5%) artificial cerebrospinal fluid (aCSF) (124 mM NaCl, 3 mM KCl, 1.2 mM NaH₂PO₄, 25 mM NaHCO₃, 2 mM CaCl₂, 1 mM MgSO₄ and 10 mM glucose, pH 7.40). The whole hippocampus was dissected out free of the subiculum or enthorinal cortex areas and the ventral part, i.e., the portion lying in the temporal part of the brain, was isolated from the dorsal one (the portion lying just behind the septum) by a cut made perpendicularly to the long hippocampal axis. The ventral hippocampi were homogenized in an ice-cold isosmotic sucrose solution (0.32 M, containing 1 mM EDTA, 1 mg/ml bovine serum albumin, and 10 mM HEPES, pH 7.4), and centrifuged at 3,000xg for 10 min; the supernatant was centrifuged again at 14,000 g for 12 min. The whole procedure was conducted at 4°C. The pellet was resuspended in 45% Percoll in KHR solution consisting of (in mM) NaCl 140, EDTA 1, HEPES 10, KCl 5, and glucose 5, and was centrifuged 14,000 g for 2 min. The synaptosomal fraction corresponds to the top buoyant layer and was collected from the tube. Percoll was removed by two washes with a KHR solution; synaptosomes were then kept on ice and used within 3 h. The synaptosomes were loaded for 20 min at 37 °C, with [methyl-³H] Choline chloride (10 µCi/ml, 122 nM). Hemicholinium-3 (10 µM) was present in all solutions up the end of the experiments to prevent choline uptake. Synaptosomes were then layered over Whatman GF/C filters and superfused (flow rate 0.8 ml/min, chamber volume 90 µl) with gassed aCSF. After a 30-min washout period, the effluent was collected (release period) in 2 min fractions for 36 min. The synaptosomes were stimulated during 2 min with 20 mM K⁺ (isomolar substitution of Na⁺ with K⁺ in the perfusion buffer) at the 5^th and 23^rd minutes after starting sample collection (S1 and S2). The tested drugs were added to the superfusion medium at the 17^th minute, therefore before S2, and remained in the bath up to the end of the experiments. When we evaluated the changes of galanin effect by the D₁-like receptor agonist SKF 38393, this was applied at the beginning of the washout period and therefore it was present during S1 and S2 in both test and control chambers, whereas galanin was added before S2 in the test chambers. A ‘mirror’ experiment was also performed to evaluate changes of the effect of SFK 38393 effect by galanin; in this case the neuropeptide was applied at the beginning of the washout period, being therefore present during S1 and S2 in both test and control chambers, whereas SKF 38393 was added before S2 in the test chambers. At the end of each experiment, aliquots (500 µl) of each sample as well as the filters from each superfusion chamber were analysed by liquid scintillation counting. The fractional release was expressed in terms of the percentage of total radioactivity present in the preparation at the beginning of the collection of each sample. The amount of radioactivity released by each pulse of K⁺ (S1 and S2) was calculated by integration of the area of the peak upon subtraction of the estimated basal tritium release. In each experiment, two synaptosome-loaded chambers were used as control chambers, the others being used as test chambers. In the test chambers, the test drug was added to the perfusion solution before S2 and the S2/S1 ratios in control and test conditions were calculated. The effect of the drug on the K⁺-evoked tritium release was expressed as percentage of change of the S2/S1 ratios in test conditions compared to the S2/S1 ratios in control conditions, in the same experiments (i.e., with the same pool of synaptosomes). When present during S1 and S2, neither galanin nor SKF 38393 significantly (P>0.05, Student’s t-test) alter the S2/S1 ratio as compared with the S2/S1 ratio obtained in the absence of these drugs. The values presented are mean ± S.E.M. of n experiments. For comparisons, statistical significance was assessed with Student’s t test using GraphPad Software (Prism, version 4.02 for Windows).

Field EPSP recordings from hippocampal slices

After decapitation under halothane anesthesia the hippocampal was dissected out of the brain on ice-cold continuously oxygenated (O₂/CO₂: 95%/5%) aCSF, as described above. Ventral and dorsal hippocampal slices (400-µm-thick, cut perpendicularly to the long axis of the hippocampus) were allowed to recover functionally and energetically for at least 1h in a resting chamber filled with continuously oxygenated (O₂/CO₂: 95%/5%) aCSF, at room temperature (22–25°C). After recovering, slices were transferred to a recording chamber (1 ml plus 5 ml dead volume) for submerged slices, and were continuously superfused (3 ml/min) at 32°C with oxygenated aCSF; the drugs were added to this superfusion solution. To minimize peptide lost due to binding to the perfusion system, all the system was superfused with BSA 0.1 mg/ml before starting any experiment. Field Excitatory Post-Synaptic Potentials (fEPSPs) were recorded as routinely (e.g. Diógenes at al., 2004) through an extracellular microelectrode (4 M NaCl, 2–6 MΩ resistance) placed in the stratum radiatum of the CA1 area. Stimulation (rectangular 0.1 msec pulses, once every 15 sec) was delivered through a concentric electrode placed on the Schaffer collateral-commissural fibbers, in the stratum radiatum near the CA3–CA1 border. The intensity of stimulus (80–200 µA) was initially adjusted to obtain a large fEPSP slope with a minimum population spike contamination. Recordings were obtained with an Axoclamp 2B amplifier and digitized (Axon Instruments, Foster City, CA). Individual responses were monitored, and averages of eight consecutive responses were continuously stored on a personal computer with the LTP program (Anderson and Collingridge, 2001). Data are expressed as mean ± SEM from n number of slices. To allow comparisons between different experiments, slope values were normalized, taking as 100% of the averaged of the five values obtained immediately before applying the test compound. The significance of differences between the mean values obtained in test and control conditions was evaluated by Student's t test. For Multiple comparisons the one-way ANOVA followed by the Bonferroni correction was used.

Drugs

Galanin was from Bachem (Weil am Rhein, Germany). (R)-(+)-7-chloro-8-hydroxy-3-methyl-1-phenyl-2,3,4,5-te trahydro-1H-3-benzazepine hydrochloride (SCH 23390), (±)-6-chloro-2,3,4,5-tetrahydro-1-phenyl-1H-3-benzazepine hydrobromide (SKF 81297), (±)-1-Phenyl-2,3,4,5-tetrahydro-(1H)-3-benzazepine-7,8- diol hydrobromide (SKF 38393) and galanin (1–13)-Pro-Pro-(Ala-Leu-)₂Ala amide (M40) were from Tocris Cookson (Ballwin, MO). Bovine serum albumin (BSA) and atropine were from Sigma (St. Louis, MO, USA). Galanin was supplied as a powder that was resuspended in TBS buffer (50 mM Tris-base, 150 mM NaCl, pH 7.60) in a 0.5 mM concentration stock solution. SCH 23390 (10 mM), SKF 38393 (10 mM) and atropine (50 mM) stock solutions were prepared in water. Aliquots of these stock solutions were kept frozen at −20°C until use.

Results

D₁ and D₅ receptors form heteromers with Gal₁ receptors but not with Gal₂ receptors

We first looked for a molecular interaction between dopamine D₁-like and Gal₁ receptors using an in vitro energy transfer assay. First, receptors were cloned as fusion proteins competent for energy transfer experiments. To ensure the fusion proteins trafficked to the correct location in the cell, we performed immunofluorescence experiments in transfected HEK cells. All fusion proteins were found to properly express and localize at the plasma membrane (Fig. 1a). Fusion of Rluc or YFP did not modify receptor function, as determined by ERK1/2 phosphorylation assays (data not shown). Next, we examined whether D₁ or D₅ and Gal₁ receptors form heteromers using the Bioluminescence Resonance Energy Transfer (BRET) technique. The BRET technique allows real-time detection of two proteins in close proximity in living cells. BRET measurements were performed in transiently co-transfected HEK cells using a constant amount of cDNA, corresponding to D₁-Rluc or D₅-Rluc receptors, and increasing amounts of cDNA, corresponding to Gal₁-YFP receptors. A positive and saturable BRET signal was obtained in cells co-expressing D₁-Rluc and Gal₁-YFP receptors, with a BRET_max of 47 ± 4 mBU and a BRET₅₀ value of 7 ± 2, or in cells co-expressing D₅-Rluc and Gal₁-YFP receptors, with a BRET_max of 71 ± 3 mBU and a BRET₅₀ value of 6 ± 1 (Fig. 1b), indicating that both D₁ and D₅ receptors formed heteromers with Gal₁ receptors. As negative controls we used, first, cells co-transfected with a constant amount of cDNA corresponding to 5HT_2B-Rluc and increasing amounts of cDNA corresponding to Gal₁-YFP receptors. Second, we also used cells co-transfected with a constant amount of cDNA corresponding to D₁-Rluc or D₅-Rluc and increasing amounts of cDNA corresponding to CB₁-YFP receptors. Only a small and linear BRET was detected (Fig 1b), indicating that the saturable BRET between D₁ or D₅ and Gal₁ represented a true complex.

Figure 1. D₁-Gal₁ and D₅-Gal₁ receptor heteromers in living cells.

(a) Confocal microscopy images of cells expressing: (top to bottom) D₅-Rluc (0.6 µg plasmid) and Gal₁-YFP (1 µg plasmid), Gal₂-Rluc (0.5 µg plasmid) and D₅-YFP receptors (1 µg plasmid), D₁-Rluc (0.5 µg plasmid) and Gal₁-YFP (1 µg plasmid) or Gal₂-Rluc (0.5 µg plasmid) and D₁-YFP (1.3 µg plasmid) receptors. Proteins were identified by fluorescence or by immunocytochemistry. D₅-Rluc, D₁-Rluc, or Gal₂-Rluc receptor immunoreactivity is shown in red, Gal₁-YFP , D₅-YFP or D₁-YFP receptor fluorescence in shown in green and co-localization is shown in yellow; scale bars, 5 µm. (b) BRET experiments were performed with cells co-expressing (red) D₅-Rluc (400 ng plasmid) or (blue) D₁-Rluc (300 ng plasmid) and Gal₁-YFP receptors (0.4 to 7 µg plasmid), Gal₂-Rluc (300 ng plasmid) and (green) D₅-YFP receptors (0.5 to 5 µg plasmid) or (purple) D₁-YFP receptors (0.5 to 4 µg plasmid), or, as negative controls, (gray) D₅-Rluc (600 ng plasmid) or (orange) D₁-Rluc (500 ng plasmid) and CB₁-YFP receptors (0.5 to 7 µg plasmid) or (black) 5HT_2B-Rluc (1 µg plasmid) and Gal₁-YFP receptors (0.5 to 5 µg plasmid). Both fluorescence and luminiscence of each sample were measured before every experiment to confirm similar donor expressions (about 150,000 luminescent units) while monitoring the increase acceptor expression (10,000–70,000 fluorescent units). The relative amount of BRET is given as the ratio between the fluorescence of the acceptor minus the fluorescence detected in cells only expressing the donor, and the luciferase activity of the donor. BRET data are expressed as means ± SD of 4–16 different experiments grouped as a function of the amount of BRET acceptor. At the top a scheme corresponding to a BRET assay is shown.

Since D₁-like and Gal₁ receptors can form heteromers, we sought to determine whether D₁-like and Gal₂ receptors could also form heteromers. Using confocal microscopy, we confirmed expression, proper trafficking of receptors and co-localization between D₁-YFP and Gal₂-Rluc receptors and between D₅-YFP and Gal₂-Rluc receptors (Fig. 1a). When we performed BRET experiments, however, we obtained a linear non-specific BRET signal in cells expressing a constant amount of Gal₂-Rluc and increasing amounts of D₁-YFP or D₅-YFP receptors (Fig. 1c), suggesting that the two pairs of receptors are not able to form heteromers. Therefore, the results indicate that D₁-like receptors show a preference for forming receptor heteromers with Gal₁ receptors.

D₁ and D₅ receptors compete for the same molecular determinants of Gal₁ receptors

Previous studies have shown that the C termini of D₁ and D₅ receptors are selectively involved in the formation of heteromers with the ligand-gated ion channels of NMDA and GABA_A receptors (Liu et al., 2000; Lee et al., 2002). We, therefore, reasoned that these same regions might interact with Gal₁ receptors. We constructed plasmids expressing the C-terminal part of the D₁ and D₅ receptors fused to glutathiol-s-transferase protein (GST-D₁CT and GST-D₅CT). We produced this protein in E. Coli and then added it to lysates from HEK-293T cells transfected with either Gal₁-YFP or Gal₂-YFP receptors. Using sepharose beads coated with glutathione we precipitated GST-D₅CT. Upon analysis of fluorescence we found that the GST-D₅CT fusion protein, but not GST alone, pulled down Gal₁-YFP receptors, but not Gal₂-YFP receptors, as demonstrated by a significant increase in fluorescence in the samples from cells expressing Gal₁-YFP, compared with samples from cells expressing YFP alone (Fig. 2a). When we tried the same experiments with GST-D₁CT, we were unable to pull down Gal₁-YFP or Gal₂-YFP (Fig. 2b). In view of the very similar results obtained in BRET experiments with the selective heteromerization of both D₁ and D₅ receptors with Gal₁ but not Gal₂ receptors, these results suggest that additional regions outside of the C-terminus play a role in forming heteromers and that there are differences between D₁ and D₅ receptors in the regions involved in heteromerization with Gal₁ receptors. BRET competition experiments were then performed to determine whether Gal₁ receptors use the same molecular determinants to heteromerize with D1 and D5 receptors. BRET was measured in cells co-expressing D₁-Rluc and Gal₁-YFP receptors (to give approximately BRET_max values) with increasing amounts of D₅ receptors. The BRET signal decreased to very low values in the presence of increasing amounts of D₅ receptors, with a complex dose-response competition curve (Fig. 3a). As the D₁-Gal₁ heteromer is disrupted by adding D₅ receptor, D₁ and D₅ receptors must share a similar interaction surface on the Gal₁ protein. To further support this hypothesis, a BRET saturation curve was performed in cells transfected with a constant amount of cDNA for the D₁-Rluc receptor, with increasing amounts of cDNA for the Gal₁-YFP receptor and with a constant amount of cDNA for D₅ receptors. Under these conditions, there was a very significant decrease in BRET_max values (23 ± 1 versus 47 ± 4 mBU; P<0.001), but not BRET₅₀ values (9 ± 2 versus 7 ± 2), compared to the BRET saturation curve in the absence of D₅ receptors (Fig. 3b), strongly suggesting that D₁ and D₅ receptors compete for the same region of Gal₁ receptors.

Figure 2. Role of the C-terminal domains of D₁ and D₅ receptors in heteromerization with Gal₁ receptor.

Extracts from cells transfected with either Gal₁-YFP or Gal₂-YFP receptors or just with YFP (see Materials and Methods) were incubated with (a) the C terminus of the D₅ receptor fused to GST (GST-D₅CT) or with just GST or (b) the C terminus of the D₁ receptor fused to GST (GST-D₁CT) or with just GST. The results of pull-down experiments (see Materials and Methods) were analyzed by measuring fluorescence. Results are expressed as means ± S.E.M. (3 independent experiments with 3 replicates) of relative fluorescence units (RFUs); **: significantly different compared to the pull down of YFP with GST-D5CT (p<0.01; repeated measures ANOVA with Bonferroni’s correction); ^###: significantly different compared to the pull down of Gal1-YFP with GST (P<0.001; repeated measures ANOVA with Bonferroni’s correction).

Figure 3. D₁ and D₅ receptors compete for binding to Gal₁ receptors.

BRET experiments were performed with cells co-expressing: (a) D₁-Rluc (300 ng plasmid) and Gal₁-YFP receptors (4 µg plasmid) and increasing amounts of D₅ receptors (0 to 5.5 µg plasmid) or (b) D₁-Rluc (300 ng plasmid), Gal₁-YFP (0.3 to 5 µg plasmid) and D₅ receptors (1.5 µg plasmid). In (a) no significant variation in luminescence due to D₁-Rluc receptors (about 150000 luminescent units) or fluorescence due to Gal₁-YFP receptors (about 10000–70000 fluorescent units) was observed by increasing D₅ receptor expression. In (b) similar luminescence due to D₁-Rluc or fluorescence due to Gal₁-YFP receptors was obtained in the absence or in the presence of D₅ receptors. The relative amount of BRET is given as the ratio between the fluorescence of the acceptor minus the fluorescence detected in cells only expressing the donor, and the luciferase activity of the donor. BRET data are expressed as means ± SD of 4–16 different experiments grouped as a function of the amount of BRET acceptor. The dashed curve represents BRET saturation curve obtained with D₁-Rluc receptor and increasing amounts of cDNA for Gal₁-YFP receptor in the absence of D₅ receptors shown in Fig. 1.

Functional characteristics of D₁-Gal₁ and D₅-Gal₁ receptor heteromers

To investigate whether D₁-like receptors can modify Gal₁ receptor function, and vice versa, we measured changes in ERK1/2 phosphorylation in the presence or absence of D₁-like and Gal₁ receptor agonists and / or antagonists. First, the D₁-like receptor agonist SKF 81297 (50 nM) time-dependently induced ERK1/2 phosphorylation in cells expressing D₁ or D₅ receptors, while galanin (100 nM) time-dependently induced ERK1/2 phosphorylation in cells expressing Gal₁ receptors (Fig. 4a). In cells expressing both D₅ and Gal₁ receptors (Fig. 4b,c) or D₁ and Gal₁ (Fig. 4d,e) receptors, SKF 81297-induced dose-response curves were not significantly modified by the presence of galanin (100 nM) (Fig. 4b,d). EC₅₀ values in cells expressing both D₅ and Gal₁ receptors were 17 ± 2 nM and 23 ± 3 nM in the absence or in the presence of galanin, respectively (non-paired t test: N.S.; n=5 in both groups). In cells expressing both D₁ and Gal₁ receptors EC₅₀ values were 7 ± 1 nM and 11 ± 1 nM in the absence or in the presence of galanin, respectively (non-paired t test: N.S.; n=5 in both groups). On the other hand, galanin-induced dose-response curves were significantly shifted to the left in the presence of SKF 81297 (50 nM) (Fig. 4c,e). EC₅₀ values were 17.1 ± 0.7 nM in the absence of SKF 81297 and 4.8 ± 0.6 nM in the presence of SKF 81297 in cells expressing both D₅ and Gal₁ receptors (non-paired t test: p<0.001; n=4 in both groups). EC₅₀ values in cells expressing both D₁ and Gal₁ receptors were 21 ± 2 nM in the absence of SKF 81297 and 6 ± 1 nM in the presence of SKF 81297 (non-paired t test: p<0.001; n=4 in both groups). These results demonstrate that D₁-like receptor agonist-activation facilitates Gal₁ receptor-mediated MAPK signaling, whereas the reverse is not true, since no significant functional effects were observed in the SKF 81297-induced dose-response curves with galanin. Importantly, in cells expressing both D₁ and Gal₂ receptors or D₅ and Gal₂ receptors, galanin-induced dose-response curves were not significantly modified by the presence of SKF 81297 (Fig. 5), suggesting that the enhancement of Gal₁ receptor-mediated MAPK signaling by D₁-like receptor agonist-activation is a biochemical property of D₁-Gal₁ and D₅-Gal₁ receptor heteromers.

Figure 4. Crosstalk between D₁-like receptors and Gal₁ receptors on ERK1/2 phosphorylation in transfected cells.

In (a) cells transfected with the cDNA corresponding to D₅ (1.5 µg, black), to D₁ (1.2 µg, white) or to Gal₁ (2 µg, gray) receptors were stimulated for the indicated times with 50 nM (black) or 70 nM (white) of the D₁-like receptor agonist SKF 81297 or with 100 nM galanin (grey). ERK1/2 phosphorylation was determined as indicated in Materials and Methods. The immunoreactive bands from 3–5 experiments were quantified and the values represent the mean ± S.E.M. of the percentage of phosphorylation relative to the basal levels found in untreated cells; * and ***: significantly different compared to the results obtained after 1 min of agonist exposure (p<0.05 and p<0.001, respectively; one-way ANOVA with Bonferroni’s correction). In (b to e) cells co-transfected with the cDNA corresponding to (b and c) D₅ (1.3 µg) and Gal₁ (1.8 µg) receptors or (d and e) D₁ (1 µg) and Gal₁ (1.8 µg) receptors were treated for 5 min with the indicated concentrations of (b and d) the D₁-like receptor agonist SKF 81297 in the absence (circles) or in the presence (triangles) of 100 nM galanin or with the indicated concentrations of galanin in absence (circles) or in the presence (triangles) of 50 nM (c) or 70 nM (d) SKF 81297. The immunoreactive bands from 4 independent experiments were quantified and the values represent the mean ± S.E.M. of phosphorylation (arbitrary units) minus the basal levels found in (b and d) SKF 81297 or (c and e) galanin untreated cells.

Figure 5. Lack of crosstalk between D₁-like receptors and Gal₂ receptors on ERK1/2 phosphorylation in transfected cells.

Cells were co-transfected with the cDNA corresponding to D₅ (1.5 µg) and Gal₂ (2 µg) receptors (a) or to D₁ (1 µg) and Gal₂ (2 µg) receptors (b). Cells were treated for 5 min with the indicated concentrations of galanin in the absence (circles) or in the presence (triangles) of 50 nM (a) or 70 nM (b) of SKF 81297. The immunoreactive bands from 4 independent experiments were quantified and the values represent the mean ± S.E.M. of phosphorylation (arbitrary units) minus the basal levels found in untreated cells.

Next, we examined the effect of heteromer formation on antagonist-modulation of agonist-induced ERK1/2 phosphorylation. The D₁-like receptor antagonist SCH 23390 (10 µM) was able to block ERK1/2 phosphorylation caused by SKF 81297 in cells expressing D₁ or D₅ receptors, while the putative non-selective galanin receptor antagonist M40 (10 µM) blocked galanin-induced ERK1/2 phosphorylation in cells expressing Gal₁ receptors (Fig. 6a). It is important to mention that M40, as well as other galanin-like peptides, have been shown to act as full agonists in some cell lines, although they are clearly antagonists in vivo (Lang et al., 2007). In our hands M40 behaved as a galanin receptor antagonist, as evidenced by the complete reversion of galanin-induced signaling. In addition, we established that, in cells only expressing D₁ or D₅ receptors signaling induced by the D₁-like receptor agonist SKF 81297 was not modified by the presence of M40 and, in cells only expressing Gal₁, signaling induced by galanin was not altered by addition of SCH 23390 (Fig. 6a). In cells co-expressing both D₅ and Gal₁ receptors (Fig. 6b) or both D₁ and Gal₁ receptors (Fig. 6c), D₁-like receptor-mediated ERK1/2 phosphorylation could be blocked by SCH 23390 but not by M40. However, galanin-induced ERK1/2 phosphorylation was counteracted by both M40 and SCH 23390 (Fig. 6b,c). This is a clear example of unidirectional cross-antagonism in a receptor heteromer (Carriba et al., 2007; Ferrada et al., 2009; Navarro et al., 2010b). Since, by definitition, an antagonist is not able to induce intracellular signaling, the more straightforward way to explain the effect of D₁-like receptor antagonist on Gal₁ receptor activation is through a direct protein-protein interaction between both receptors.

Figure 6. D₁-like receptor antagonist-mediated blockade of galanin-induced ERK1/2 phosphorylation in cells expressing D₁-like and Gal₁ receptors.

In (a), cells were transfected with the cDNA corresponding to D₅ (1.5 µg, black), D₁ (1.2 µg, white) or Gal₁ receptors (2 µg, grey) and were stimulated with the D₁-like receptor agonist SKF 81297 (70 nM) or with galanin (100 nM), in the presence or in the absence of the D₁-like receptor antagonist SCH 23390 (10 µM) or the Gal₁ receptor antagonist M40 (10 µM); ***: significantly different compared to the effect of SKF 81297 alone (black and white columns) or to the effect of galanin alone (grey columns) (p<0.001; one-way ANOVA with Bonferroni’s correction). In (b and c), cells co-transfected with the cDNA corresponding to D₅ (1.3 µg) and Gal₁ receptors (1.8 µg) (b) or to D₁ (1 µg) and Gal₁ (1.8 µg) receptors (c) were treated with SCH 23390 (10 µM), M40 (10 µM), SKF 81297 (70 nM) or galanin (100 nM) alone or in combination; ***: significantly different compared to the effect of SKF 81297 alone (in cells treated with SKF 81297) or to the effect of galanin alone (in cells treated with galanin) (p<0.001; one-way ANOVA with Bonferroni’s correction). In all cases, cells were treated for 5 min with the indicated concentrations of agonists and 20 min prior to the addition of agonists with the indicated concentrations of antagonists. The inmunoreactive bands from 4–5 experiments were quantified and the values represent the mean ± S.E.M. of the percentage of phosphorylatyon relative to the basal levels found in untreated cells (100 %).

D₁-like-Gal₁ receptor heteromers are expressed in the rat ventral hippocampus

In view of the cross-antagonism clearly observed in the transfected cells, we decided to use a similar approach to seek biochemical evidence (“biochemical fingerprint”) for the existence of D₁-like-Gal₁ receptor heteromers in the brain (see Ferré et al., 2009). Therefore, to test if D₁-Gal₁ or D₅-Gal₁ receptor heteromers exist in the brain, we isolated rat ventral and dorsal hippocampal slices and compared the ability of the D₁-like receptor antagonist SCH 23390 to block the effect of galanin on ERK1/2 phosphorylation. Slices were incubated with galanin in the absence or in the presence of either SCH 23390 or the galanin receptor antagonit M40. In the ventral hippocampus, the results reproduced the cross-antagonism found in transfected cells (Fig. 7). ERK1/2 phosphorylation induced by galanin (300 nM) was not only blocked by M40 (10 µM) but also by SCH23390 (10 µM). In contrast, in dorsal hyppocampus slices, SCH23390 (10 µM) failed to antagonize the effect of galanin (Fig. 7). These results provide strong evidence for the existence of D₁-like-Gal₁ receptor heteromers in the ventral hippocampus.

Figure 7. D₁-like receptor antagonist-mediated blockade of galanin-induced ERK1/2 phosphorylation in rat hippocampal slices.

Slices from dorsal (black) or ventral (white) hippocampus were treated for 10 min with medium, SCH 23390 (10 µM) or M40 (10 µM) prior to the addition of galanin (300 nM) and a further incubation period of 10 min. The inmunoreactive bands from 4 slices from two different animals were quantified and the values represent the mean ± S.E.M. of the percentage of phosphorylation relative to the basal levels found in untreated slices (100 %). * and **: significantly different compared to the effect of galanin alone (p<0.05 and p<0.01, respectively; one-way ANOVA with Bonferroni’s correction).

The role of D₁-like and Gal₁ receptor co-activation on K⁺-induced [³H]ACh release in synaptosomes from rat ventral hippocampus

Having established that D₁-like-Gal₁ receptor heteromers occur in the ventral hippocampus, we looked for their functional role by first analyzing the effect of a D₁-like agonist and galanin on K⁺-induced [³H]ACh release in isolated synaptosomes from rat ventral hippocampus. The D₁-like receptor agonists SKF 81297 and SKF 38393 have a similar affinity for D₁ and D₅ receptors. The major difference between the two agonists is a significantly higher selectivity for D₁ versus dopamine D₂ receptors and D₁ versus serotonin 5-HT_2A receptors of SKF 38393 compared to SKF 81297 (Seeman et al, 1994; Neumeyer et al., 2003). Since selectivity was a major concern when dealing with hippocampal tissue, we decided to shift to SKF 38393 as the D₁-like receptor agonist in the studies of ACh release in synaptosomes and the electrophysiological studies in slices. Neither galanin, at low nanomolar concentrations (30–100 nM) in the range used by Wang et al. (1999) in rat cortical slices and cortical synaptosomal preparations, nor the D₁-like receptor agonist SKF 38393 (20–100 nM) significantly (P>0.05, n=3–6) affected K⁺-induced ACh release, as assessed by modifications of the S2/S1 ratio upon addition of the agonists before S2. However, prior addition of SKF 38393 (20 nM; added before S1 and being present during S1 and S2) triggered an excitatory effect (P<0.05, n=6) of galanin (30 nM; only added before S2) on evoked ACh release (Fig. 8a). On the other hand, no significant functional effects where observed with the reverse protocol, since adding galanin (30 nM) before S1 did not influence the absence of effect of SKF 38393 (20 nM, only added before S2) (Fig. 8b). These results nicely correlate with the functional results obtained in cells expressing D₁ or D₅ and Gal₁ receptors, showing the selective enhancement of Gal₁ but not Gal₂ receptor-mediated MAPK signaling by a D₁-like receptor agonist. Therefore, the results strongly suggest that D₁-Gal₁ or D₅-Gal₁ receptor heteromers are present in ventral hippocampal cholinergic terminals where they modulate ACh release.

Figure 8. Effect of a D₁-like receptor agonist and galanin on K⁺-induced [³H]ACh release from ventral hippocampal synaptosomes.

In (a), dopamine receptors were activated (right column) by preincubation with the agonist SKF 38393 before addition of galanin. In (b), galanin receptors were activated (right column) by preincubation with galanin before addition of SKF 38393. Ordinates represent the S2/S1 ratios as percentage of the control value in the same experiments (see Materials and Methods). Drug conditions during S1 and S2 are indicated below each bar. 100% in the ordinates represents the S2/S1 ratio in the absence of the test drug, i.e., in the absence of galanin (a) or in the absence of SKF 38393 (b), using the same synaptosomal batch. An S2/S1 ratio close to 100% represents, therefore, absence of effect of the test drug (galanin in (a) or SKF 38393 in (b)). Values are mean ± S.E.M (n=3–6). 100% in (a) corresponds to 0.76 ± 0.046 and in (b) to 0.70 ± 0.029. The presence of SKF 38393 (a) or of galanin (b) during S1 and S2 did not significantly affect S2/S1 ratios as compared with those obtained in the absence of any drug *: p<0.05; NS: P>0.05 (Student’s t test).

The role of D₁-like and Gal₁ receptor co-activation on rat ventral hippocampus synaptic transmission

To identify whether D₁-like-Gal₁ receptor interactions affect excitatory synaptic transmission in the hippocampus, we evaluated the effect of galanin on excitatory postsynaptic potentials (EPSPs) in hippocampal slices (Fig. 9a) in the absence or presence of the dopaminergic receptor agonist SKF 38393. As illustrated in Fig. 9b,e, when galanin (30 nM) was applied alone to ventral hippocampal slices there was a statistically significant (P<0.05, n=9) inhibition (21 ± 2.6 %) of the slope of fEPSP. On the other hand, SKF 38393 (20 nM) was virtually devoid of effect (n=7) on the slope of fEPSP (Fig. 9c,e). However, in the presence of SKF 38393, the effect of galanin was reversed and it produced a significant increase of 15.4 ± 2.4 % (P<0.05, n=8) in the slope of fEPSPs (Fig. 9d, f). These results indicate a synergistic effect when both D₁-like and Gal₁ receptors are co-stimulated by agonists and match those results obtained in synaptosomal preparations when measuring ACh release and those results obtained in transfected cells and in ventral hippocampal slices while measuring EPK phosphorylation. Moreover, blockade of D₁-like receptors with SCH 23390 (1 µM; added 30 min before SKF 38393) completely counteracted the effect of SKF 38393 (Fig. 9d,f). Indeed, in the presence of SCH 23390 (1 µM) and SKF 38393 (20 nM), galanin (30 nM) decreased (P<0.05, n=6) the slope of fEPSPs by 21.2 ± 3.4 % (Fig. 9d), an effect similar to that observed when galanin was applied to the slices alone (Fig. 9b,f).

Figure 9. Effect of co-activation of D₁-like and galanin receptors on galanin-mediated modulation of synaptic transmission in the ventral hippocampus.

(a) schematic representation of a transverse hippocampal slice with the electrode configuration used to record fEPSPs in the CA1 apical dendritic layer (stratum radiatum) evoked by electric stimulation (S₀) of the Schaffer fibers. (b) Averaged time courses of changes in fEPSP slope induced by application of 30 nM galanin alone. (c) Averaged time course of changes in fEPSP slope induced by application of 20 nM SKF 38393 alone. (d) Averaged time courses of the effect of galanin (30 nM) in the presence of the D₁-like receptor agonist SKF 38393 (20 nM) (●) or in the presence of both SKF 38393 (10 nM) and the D₁-like receptor antagonist SCH23390 (1 µM) (○). SKF 38393 was applied at least 30 min before galanin application, and SCH 23390 was applied 30 min before SKF 38393 application. In (e) recordings obtained from representative experiments, where each trace is the average of eight consecutive responses obtained in absence (1) and presence (2) of galanin (30 nM) (left panel), in absence (3) and presence (4) of SKF 38393 (20 nM) (middle panel) and in absence (5) and presence (6) of galanin (30 nM) when the slice was incubated with SKF 38393 (20 nM) (right panel), are shown D₁-like; each trace is composed of the stimulus artifact, followed by the presynaptic volley and the fEPSP; superimposed recordings were obtained from the same slice at the time points indicated in panels b–d. Note the inhibitory effect of galanin in b) (absence of SKF 38393) and facilitatory effect in d (presence of SKF 38393). In (f), comparison between the averaged effects of galanin on hippocampal synaptic transmission in presence of SKF 38393 and in presence of both SKF 38393 and SCH 23390. The ordinates shows the percent change of fEPSP slope induced by galanin (30 nM) 50–60 min after its application to hippocampal slices not treated or treated with SKF 38393 and treated with both SKF 38393 and SCH 23390, as indicated below each bar. θ: p<0.05 (one-way ANOVA with Bonferroni’s correction) as compared with absence of galanin in the same slices, φ: p<0.05 (one-way ANOVA with the Bonferroni’s correction) as compared with galanin alone. All values are mean ± SEM; 100% (averaged fEPSP slopes at times −10 to 0): a) −0.69 ± 0.073 mV/msec, n = 8 (●), −0.66 ± 0.103 mV/msec, n = 6 (○); b) −0.69 ± 0.023 mV/msec, n = 9; c) −0.64 ± 0.041 mV/msec, n = 7)

Based on our results on the modulation of ACh release from isolated nerve terminals (see above) and previous evidence that dopamine and galanin receptors regulate septo-hippocampal cholinergic neurotransmission, we hypothesised that the cross-talk between galanin and dopamine receptors involved in the modulation of hippocampal excitatory transmission resulted from modulation of cholinergic neurotransmission. To test this hypothesis, we used the muscarinic cholinergic receptor antagonist atropine (5 µM), which by itself did not significantly modify fEPSP when applied to ventral hippocampal slices (Fig. 10b). The application of SKF 38393 (20 nM) after previous application (at least 30 min before) of atropine also did not significantly affect synaptic transmission (Fig. 10b). However, when galanin was added a significant inhibition (P<0.05, n=6) of the slope of fEPSP was observed (Fig. 10a,b). This inhibition (21 ± 5%) was similar to the inhibition obtained when galanin was applied in the absence of any drug (18 ± 0.9%, Fig. 8a,d), demonstrating a cholinergic-independent depressant effect of galanin, but a cholinergic-dependent facilitatory action of galanin that requires D₁-like receptor activation. These results suggest that D₁-like-Gal₁ receptor heteromers localized in cholinergic terminals influence excitatory synaptic transmission in the ventral hippocampus. Finally, we performed fEPSP measurements using slices of dorsal hippocampus. Application of galanin (30 nM) to dorsal hippocampal slices had no significant effect on fEPSP slope (Fig. 11a). Application of SKF 38393 (20 nM) was also devoid of any effect on fEPSP slope (Fig. 11b). Furthermore, previous addition of SKF 38393 (20 nM; 30 minutes before) did no trigger any effect of galanin on fEPSPs (Fig. 11c,d). These results agree with the selective existence of D₁-like-Gal₁ receptor interactions in the ventral versus the dorsal hippocampus, as indicated by the ERK1/2 phosphorylation experiments in hippocampal slices.

Figure 10. Effect of muscarinic receptor blockade on the dopamine-dependent galanin-mediated modulation of synaptic transmission in the ventral hippocampus.

In (a), upper graph, averaged time courses of the effect of galanin (30 nM) in the presence of both the D₁-like receptor agonist SKF 38393 (20 nM) and the muscarinic acetylcholine receptors antagonist atropine (5 µM). SKF 38393 was applied at least 60 min before galanin, and atropine was applied 30 min before SKF 38393. Lower graph are traces obtained with a representative experiment; each trace is the average of eight consecutive responses obtained immediately before (1) and during (2) galanin application, and is composed of the stimulus artifact, followed by the presynaptic volley and the fEPSP. In (b), comparison between the averaged effects of galanin (30 nM for 50–60 min) in the absence of drugs and in presence of both SKF 38393 and atropine. The averaged effects of atropine and both atropine and SKF 38393 are also shown; θ: p<0.05 (Students’ t test) as compared with absence of galanin in the same slices; φ: p<0.05 (Students’ t test) as compared with both atropine and SKF 38393 present in the same slices. All values are mean ± SEM; 100% (averaged fEPSP slopes at times −10–0): −0.60 ± 0.037 mV/msec, n = 6 (a).

Figure 11. Lack of effect of galanin on synaptic transmission in the dorsal hippocampus.

(a) and (b) show the averaged time course of changes in fEPSP slope induced by application of 30 nM galanin (a) or 20 mM SKF 38393 (b). In (c), averaged time courses of the effect of galanin (30 nM) in the presence of the D₁-like receptor agonist SKF 38393 (20 nM). SKF 38393 was applied at least 30 min before galanin; ordinates show the percent change of fEPSP slope induced by galanin (30 nM) 50– 60 min after its application to hippocampal slices non-treated and treated with SKF 38393, as indicated below each bar. All values are mean ± SEM; 100% (averaged fEPSP slopes at times −10–0): −0.55 ± 0.070 mV/msec, n = 5 (a), −0.58 ± 0.048 mV/msec, n = 3 (b), −0.55 ± 0.064 mV/msec, n = 3 (c). In (d), comparison between the averaged effects of galanin in presence and absence of SKF 38393.

Discussion

By using a multi-disciplinary approach, we provide several important mechanistic and functional insights into the role of galanin and dopamine on regulation of ACh release in the hippocampus. We show, for the first time, that dopamine D₁-like receptors form heteromers with Gal₁ but not with Gal₂ receptors in transfected cells and in rat ventral hippocampus. Within the D₁-Gal₁ and D₅-Gal₁ receptor heteromer, dopamine receptor activation and blockade potentiate and counteract, respectively, MAPK activation induced by stimulation of Gal₁ receptors, while Gal₁ receptor ligands do not modify D₁-like receptor-mediated MAPK activation. We also demonstrate that dopamine and galanin work in concert to modulate cholinergic neurotransmission in the ventral hippocampus and that this modulation could occur via heteromers between D₁ or D₅ receptors and Gal₁ receptors.

Using an in vitro cell culture system we demonstrated by BRET the ability of both D₁ and D₅ receptors to form heteromers with Gal_1, but not Gal₂ receptors. This is not surprising if we consider that these two galanin receptors have relatively low amino acid similarity (Branchek et al., 2000). While both D₁ and D₅ receptors were able to compete for their heteromerization with the Gal₁ receptor, only the C terminus of the D₅ receptor pulled down the whole Gal₁ receptor from membrane preparations of transfected cells. On the one hand, these results suggest that additional regions outside of the C-terminus play a role in forming heteromers and that there are differences between D₅ and D₁ receptors in the regions involved in heteromerization with Gal₁ receptors. On the other hand, our results strongly suggest that D₁ and D₅ receptors compete for the same region of Gal₁ receptors.

One of the main challenges in the study of membrane protein complexes is their identification in native tissues. Solubility issues and unreliable anti-bodies make co-immunoprecipitation experiments difficult to interpret and current spectroscopic approaches, with few exceptions, lack the resolution for an in situ approach at the single molecule level. These limitations, thus, require indirect approaches to validate the presence of such membrane complexes, such as the determination of a biochemical property of the receptor heteromer, which can be used as a “biochemical fingerprint” (Ferré et al., 2009). The cross-antagonism in which a D₁-like receptor antagonist is able to block the effect of a Gal₁ receptor agonist is very difficult to explain by a mechanism not involving receptor heteromerization, taking into account that an antagonist does not induce intracellular signaling. This cross-antagonism was therefore used as a “biochemical fingerprint” of the D₁-like-Gal₁ receptor heteromer. Using these criteria and measuring MAPK activation as an endpoint, we were able to identify D₁-like-Gal₁ receptor heteromers in the ventral, but not the dorsal, hippocampus.

Although the existence of Gal₁ receptors on septo-hippocampal cholinergic neurons has been previously questioned (Miller et al., 1997), our observations of the same qualitative cross-talk in signaling in synaptosomal preparations as in cells expressing D₁-like and Gal₁ receptors strongly suggests that functional Gal₁ receptors are present in cholinergic terminals of the ventral hippocampus. As mentioned above, in transfected cells, D₁-like receptor stimulation potentiates the effects of Gal_1, but not Gal_2, receptor activation, but Gal₁ receptor stimulation does not modify D₁-like receptor-mediated signaling. In hippocampal synaptosomal preparations, at nanomolar concentrations, neither galanin nor a D₁-like receptor agonist produced any modification of K⁺-induced ACh release. Nevertheless, previous activation of D₁-like receptors triggered a facilitatory effect of galanin. Also as in transfected cells, galanin did not modify the lack of effect of a D₁-like receptor agonist. Since D₅ predominates over D₁ receptors in the hippocampus (Ciliax et al., 2000) and D₅ receptors have been previously shown to be involved in the modulation of hippocampal ACh release (Hersi et al., 2000; Laplante et al., 2004b), D₅ is probably the main D₁-like receptor subtype forming heteromers with Gal₁ receptors in cholinergic terminals of the ventral hippocampus.

In previous studies, galanin generally showed an inhibitory effect on hippocampal cholinergic neurotransmission (Fisone et al., 1987; Ögren et al., 1998; Laplante et al., 2004a). However, most of these studies were performed with in vivo microdialysis techniques using much higher (micromolar) concentrations of galanin than in the present experiments (Ögren et al., 1998; Laplante et al., 2004a) and with artificially increased extracellular concentrations of ACh due to the addition of acetylcholinesterase inhibitors in the perfusion medium. The use of acetylcholinesterase inhibitors in the dialysis medium has raised concerns about the possibility of not only quantitative but also qualitative artifactual results (Acquas and Fibiger, 1998; DeBoer and Abercrombie, 1996). At the level of the Shaffer-CA1 glutamatergic synapses of the ventral hippocampus, a low (nanomolar) concentration of galanin was inhibitory providing that dopamine receptors were not activated. This result is in accordance with the expression of Gal₁ receptors in the CA1 area of the ventral hippocampus (O’Donnell et al., 1999). In fact, we found galanin to be completely ineffective in the dorsal hippocampus. This cholinergic-independent depressant effect of galanin could be related to its ability to decrease neuronal hippocampal glutamatergic neurotransmission (Zini et al., 1993; Mazarati et al., 2000). Also, galanin has been reported to inhibit LTP in the Shaffer-CA1 glutamatergic synapses (Sakurai et al., 1996). The D₁-like receptor agonist, that was ineffective when administered alone, turned an inhibitory effect of galanin into an excitatory effect, and this interaction depended on cholinergic neurotransmission, since it was completely blocked by a muscarinic ACh receptor antagonist. From our results from ventral hippocampal synaptosomal preparations and slices, a model of the role of galanin in the Shaffer-CA1 synapses of the ventral hippocampus can be proposed: an isolated increase in the activity of the septo-hippocampal cholinergic input produces a modest release of ACh and galanin. This modest release of galanin would, nevertheless, be sufficient to inhibit the excitability of glutamatergic synapses by acting on pre- or postsynaptic galanin receptors. However, upon a concomitant increase in the activity of the VTA-hippocampal dopaminergic input, coactivation of D₁-like and galanin receptors localized in cholinergic terminals induces a strong release of ACh, which overcomes the inhibitory role of galanin and leads to increased excitability of the glutamatergic synapses.

The interactions reported here occur in the ventral but not in the dorsal hippocampus. These two hippocampal areas have differential efferent connections with the rest of the brain, such that the dorsal hippocampus is primarily connected with the neocortex, while the ventral hippocampus is connected to subcortical structures, such as the hypothalamus and the amygdala (Nabber and Witter, 1998). Since both the amygdala and the hypothalamus control the activity of the hypothalamus-pituitary-adrenal axis, it is therefore not a surprise that a major function of the ventral hippocampus is the processing of information related to emotion-related behaviours, as increasing evidence now indicates (see Segal et al., 2010). Interestingly, injection of acetylcholine into the ventral, but not into the dorsal, hypocampus, reduces anxiety (Degroot and Treit, 2002). One can, therefore, speculate that the cholinergic-dependent facilitatory action of galanin upon excitatory Schaffer-CA1 synapses (a last relay of the excitatory output of the hippocampus) may influence the control of anxiety and emotional memory.

Altogether, our results strongly suggest that D₁-like-Gal₁ receptor heteromers that are localized in cholinergic nerve terminals play an important role in the modulation of cholinergic neurotransmission in the ventral hippocampus. Receptor heteromers are becoming the focus of extensive research in the field of GPCRs and we are just starting to understand the mechanisms involved in heteromerization and its functional meaning (Boulenger et al., 2005; Ferré et al., 2007; Dalrymple et al., 2008; Milligan, 2009; Roszenfeld and Devi, 2010). The present study provides a clear example of a receptor heteromer acting as a processor that integrates signals of different neurotransmitters and modulates cell signaling and neuronal function (Ferré et al., 2007). Since receptor heteromers are increasingly being considered as pharmacological targets (George et al., 2002; Ferré et al., 2010), D₁-Gal₁ and D₅-Gal₁ receptor heteromers could be considered as targets for drugs useful in Alzheimer’s disease, in view of the involvement of the septo-hippocampal cholinergic system in this disease (Ögren et al., 1998; Mitsukawa et al., 2008). Importantly, D₁, D₅ and Gal₁ receptors are also co-localized in brain areas other than the hippocampus, such as the mesencephalic dopaminergic nuclei substantia nigra and the ventral tegmental area (VTA) (Schilstrom et al., 2006; Picciotto, 2008). If D₁-like-Gal₁ receptor heteromers are also present in the mesencephalic dopaminergic cells, they could be targets for the treatment of dopamine-related neuropsychiatric disorders, including drug addiction. Finally, the ability of galanin receptors to heteromerize with other GPCRs in other regions of the CNS could explain pharmacological findings that have so far been difficult to explain, such as the well-known biphasic dose-dependent effect of galanin on nociception (Xu et al., 2008).