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Original Research ARTICLE

Front. Mol. Neurosci., 21 September 2017 | https://doi.org/10.3389/fnmol.2017.00299

The Serotonin Receptor Subtype 5b Specifically Interacts with Serotonin Receptor Subtype 1A

Sabine Niebert1, Gijsbert J. van Belle2, Steffen Vogelgesang3,4, Till Manzke3,4 and Marcus Niebert3,4*
  • 1Department of Maxillofacial Surgery, University Medical Center, Göttingen, Germany
  • 2Institute of Cardiovascular Physiology, University Medical Center, Göttingen, Germany
  • 3Institute of Neuro- and Sensory Physiology, University Medical Center, Göttingen, Germany
  • 4Center Nanoscale Microscopy and Molecular Physiology of the Brain (CNMPB), University Medical Center, Göttingen, Germany

Previously, we described the dysregulation of serotonin (5-HT) receptor subtype 5b (5-ht5b) in a mouse model of Rett syndrome (RTT). 5-ht5b has not been extensively studied, so we set out to characterize it in more detail. Unlike common cell surface receptors, 5-ht5b displays no membrane expression, while receptor clusters are located in endosomes. This unusual subcellular localization is at least in part controlled by glycosylation of the N-terminus, with 5-ht5b possessing fewer glycosylation sites than related receptors. We analyzed whether the localization to endosomes has any functional relevance and found that 5-ht5b receptors can specifically interact with 5-HT1A receptors and retain them in endosomal compartments. This interaction reduces 5-HT1A surface expression and is mediated by interactions between the fourth and fifth trans-membrane domain (TMD). This possibly represents a mechanism by which 5-ht5b receptors regulate the activity of other 5-HT receptor.

Introduction

G-protein coupled receptors (GPCRs) make up ~2% of all cellular proteins and constitute one of the most important pharmaceutical drug targets. With all their diversity, GPCRs share some defining features, e.g., they are composed of seven trans-membrane domains (TMD) with three extracellular and four intracellular loops, and many receptors need to form homo- or heterodimers to become functional active (Gurevich and Gurevich, 2008; Schwenk et al., 2010; Pellissier et al., 2011). The receptors relate extracellular signals by activating G-proteins acting on either one of the main effectors calcium (Gq via Phospholipase C) or cyclic adenosine monophosphate (cAMP). cAMP can be up- or down-regulated via stimulatory (Gs) or inhibitory (Gi/G0) G-proteins who activate or inhibit the adenylate cyclase, respectively. Increases in cAMP may directly activate cyclic nucleotide gated (CNG) ion channels (Kaupp and Seifert, 2002) or protein kinase A (PKA; Meinkoth et al., 1993). Intracellular sensors for cAMP like exchange protein activated by cAMP (EPAC; Bos, 2006) or popeye domain-containing proteins (Popdc, Simrick et al., 2013) function through small GTPases.

Serotonin (5-HT) is a widespread neurotransmitter in the nervous systems, with numerous functions in sensory-motor, autonomic and behavioral systems (Azmitia, 2001). It is also a hormone and paracrine factor in non-neural tissues (Matsuda et al., 2004; Slominski et al., 2005). In mice, 5-HT receptors comprise seven groups with multiple subtypes (5-HT1A/B/D/F, 5-HT2A/B/C, 5-HT4, 5-ht5a/b, 5-HT6 and 5-HT7; Hoyer et al., 2002) for a total of 12 GPCRs, while 5-HT3A/B acts as an ion channel. In humans, four additional 5-HT receptors exist that do not have a known ortholog in mice: 5-HT1E is another GPCR, while 5-HT3C/D/E form ion channels.

While many 5-HT receptors have been extensively studied (Niebert et al., 2011; Pellissier et al., 2011; Renner et al., 2012), our knowledge of 5-ht5 receptors is rather limited. Rodents have been shown to possess two functional 5-ht5 receptor subtypes, 5-ht5a (Plassat et al., 1992) and 5-ht5b (Matthes et al., 1993), with their expression being restricted to the brain (Rees et al., 1994). The existence of both receptors was confirmed for humans (Rees et al., 1994; Grailhe et al., 2001; Nelson, 2004), which possess a functional gene for 5-ht5a, while the coding sequence of the 5-ht5b subtype is interrupted by several stop codons and insertional mutations, making the gene apparently non-functional.

5-ht5b is expressed in many regions throughout the murine brain like bulbus olfactorius, hippocampus, or cerebellum at low levels. However, 5-ht5b was found to be upregulated under the control of ATF-7 in mice undergoing social stress (Maekawa et al., 2010). Also, 5-ht5b dysregulation was described in mouse models of Rett syndrome (RTT), a severe neurodevelopmental disorder caused by mutations in the transcription factor MeCP2. We found 5-ht5b to be developmentally regulated in the brainstem of Mecp2−/y mice, where it showed 75-fold upregulation (Vogelgesang et al., 2017), while 5-ht5b was also increased in astrocytes of Mecp2308/y mice (Delépine et al., 2015). We showed that a full length as well as a truncated protein of 5-ht5b can be detected by Western blot in murine brain lysates (Vogelgesang et al., 2017). Truncation of receptors has been described many times, but previously identified truncated GPCRs were predominantly retained in the endoplasmic reticulum (ER; Karpa et al., 2000; Leung et al., 2007; Gonzalez et al., 2011).

5-ht5b’s massive dysregulation in a disease model for RTT prompted us to more closely investigate the reasons for and the physiological significance of its subcellular localization.

Materials and Methods

Ethical Statement

The experimental procedures were performed in accordance with European Community (EU Directive 2010/63/EU for animal experiments) and National Institutes of Health guidelines for the care and use of laboratory animals. The study was approved by the Georg-August-University, Göttingen and the approval ID T12/18 was assigned to this work.

Animals

C57BL/6J mice were kept in a temperature- and humidity-controlled 12 h light-dark cycle and had free access to water and standardized pellet food. The Mecp2 knockout mouse (Mecp2/y), strain B6.129P2(C)-Mecp2tm1-1Bird (Guy et al., 2001) obtained from The Jackson Laboratory (Bar Harbor, ME, USA) was maintained on a C57BL/6J background. For this work we used wild-type and hemizygous Mecp2+/− females.

Cell Culture, Transfection and Plasmids

Murine neuroblastoma cell line N1E-115 was obtained from the American Type Culture collection (ATCC). Cells were grown in Dulbecco’s modified Eagle’s medium (DMEM) containing 10% fetal calf serum (FCS) and 1% penicillin/streptomycin at 37°C under 5% CO2.

For transient transfection, cells were seeded in cell culture dishes and transfected with indicated plasmids using Lipofectamine2000 Reagent (Invitrogen) according to the manufacturer’s instruction.

Primary neurons were obtained from dissociated hippocampi as detailed in Revelo et al. (2014). In brief, hippocampi were extracted from 1 day-old animals. They were incubated for 1 h in enzyme solution (10 ml DMEM, 2 mg cysteine, 100 mM CaCl2, 50 mM EDTA and 25 U papain, equilibrated with carbogen for 10 min, and sterile filtered). Before mechanical dissociation, cells were washed thoroughly with HBSS (Invitrogen, Waltham, MA, USA) and were incubated for 15 min in inactivating solution (2 mg albumin and 2 mg trypsin inhibitor in 10 ml FCS-containing DMEM medium). Sterilized coverslips were coated overnight with 1 mg/ml poly-L-lysine and were incubated with plating medium (MEM supplemented with 10% horse serum, 3.3 mM glucose and 2 mM glutamine). Neurons were plated at a concentration of ~30,000/cm2 and were left to adhere for 1–4 h. After adhesion, the medium was changed to Neurobasal-A medium (Gibco, Life Technologies, Carlsbad, CA, USA) containing 1:50 B27 supplement (Gibco) and 1:100 GlutaMAX (Gibco). Neurons were kept in culture at 37°C and 5% CO2.

Expression constructs for 5-HT receptors 5-HT1A and 5-HT7 with either immuno- (HA/myc) or fluorescent tags have been described previously (Renner et al., 2012), while 5-HT receptors 5-HT2C, 5-HT4, 5-ht5a, 5-ht5b and 5-HT6 were generated from murine corresponding deoxyribonucleic acid (cDNA). Brain tissue was explanted and used for total ribonucleic acid (RNA) isolation with the OLS RNA kit (OLS, Germany) according to the manufacturer’s instructions. The total RNA was used in one-step RT-PCR (Invitrogen) and resulting PCR fragment was cloned into pTarget expression vector (Promega). Primer sequences are given in Table 1. To obtain a C-terminal fluorophore fusion construct, the receptor and the fluorophores CFP, GFP, YFP or mRFP/mCherry were amplified individually, and fusion PCR was used to combine the cDNAs. The resulting PCR fragment was cloned into the pTarget expression vector (Promega). To test the hypothesis of a truncated 5-ht5b receptor, we amplified the unlabeled and the mCherry fusion construct and cloned the fragments into pTarget. The truncated 5-ht5b comprises the nucleotides from position 520 to 1113. As a control, a truncated 5-HT7 was prepared in the same way. The truncated 5-HT7 comprises the nucleotides from position 520 to 1347. Correct sequences of all constructs were determined by sequencing.

TABLE 1
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Table 1. List of primers used in this study for cloning.

Generation of Glycosylation-Deficient 5-HT1A Constructs

Wild type 5-HT1A can be glycosylated at four positions (N10, N11, N24, N30) at the N-terminus. Following the glycosylation experiments on 5-ht5a, we used site-directed mutagenesis (Quickchange II, Agilent) to change each individual Asparagine to Serine (Dutton et al., 2008). To generate clones with multiple exchanges, we performed subsequent rounds of mutagenesis. Primers used for mutagenesis are given in Table 1 and correct sequences of all constructs were determined by sequencing.

Generation of Hybrid Receptors

The modular structure of the GPCRs facilitates easy exchange of domains between receptors, which has previously been used successfully to generate versions with completely new characteristics (Conklin et al., 2008). 5-HT receptors are composed of seven TMD, which are connected by three extra- (ECL) and three intra-cellular loops (ICL). The extra-cellular N-terminus takes part in ligand attraction, while the intra-cellular C-terminus often, but not always features a PDZ-like domain and takes part in membrane anchoring or protein binding. The problem with this approach is the difficulty to predict domain boundaries, as incorrectly chosen domains may prevent correct folding and therefore render the new hybrid receptor functionless. As we employed this strategy multiple times, we took care to validate the correct function of the new hybrid receptors. Our first quality check was their production of a distinct staining, be it intracellular or membrane bound. All variants that showed a diffuse staining were assumed to be incorrectly folded and were not used for further studies. As long as the receptor showed at least some membrane localization, we also tested the hybrid receptor for its reaction to its natural ligand 5-HT.

DNA sequences coding for TMDs were identified using TMHMM server 2.0 (Krogh et al., 2001). Hybrid receptors were generated using fusion PCR. Therefore, the DNA sequences to be fused were separately amplified by PCR using specific primers, introducing a small overlapping DNA region. After purification of both PCR products by gel extraction, 10 ng of each DNA was used as template for a subsequent fusion PCR using primers specific for the full-length hybrid open reading frame. The primers used for generation of different variants of Htr1a-Htr5b hybrid receptor variants are given in Table 1.

RT-PCR

The total RNA of homogenized tissue from specific brain regions was isolated using the Trizol® method according to manufacturer’s instructions (GibcoBRL) and its concentration was determined using the nanodrop ND-1000 spectrophotometer followed by its quality and integrity measurement by electrophoresis on RNA 6000 LabChip® kit (Agilent 2100 Bioanalyzer). The RNA was transcribed into the cDNA using the iScript cDNA Synthesis Kit (BioRad). The primer pairs used for RT-PCR are the same used previously for quantitative RT-PCR (Vogelgesang et al., 2017).

Immuno-Staining Procedures

To obtain tissue, mice (P40) were deeply anesthetized with isoflurane (1-Chloro-2,2,2-trifluoroethyl-difluoro-methylether, Abbott, Germany) until they were unresponsive to pain stimuli. A thoracotomy was performed and animals were transcardially perfused with 50 ml of 0.9% NaCl followed by 200 ml of 4% phosphate-buffered formaldehyde (10 ml/min). The brain was removed and post-fixed for 4 h with the same fixative at 4°C. Whole brains were stored in 1% formaldehyde in PBS at 4°C. Before sectioning, brains were equilibrated in HEPES buffer (7, 5 g NaCl, 0.3 g KCl, 0.06 g KH2PO4, 0.13 g Na2HPO4, 2 g Glucose, 2.4 ml 10 mM HEPES, 0.1 g MgCl2, 0.05g MgSO4, 0.165 g CaCl2, pH 7.4) for 48 h, cryoprotected in 15% sucrose in PBS for 24 h followed by equilibration in 30% sucrose in PBS for 24 h at 4°C, and then frozen at −80°C. Series of 30 μm thick brain sections were cut using a freezing microtome (Frigocut, Reichert-Jung, Germany). Sections were stored in HEPES buffer. All buffers were supplemented with a small amount of sodium azide.

The polyclonal antibody against the murine 5-ht5b receptor was generated by immunizing rabbits with a 15mer peptide representing the C-terminus of the receptor (NP_034613.1; NH2-KNYNNAFKSLFTKQR-COOH). Peptides were coupled to keyhole limpet hemocyanin (KLH) and 300 μg KLH-coupled peptide in Hunter’s adjuvant (TiterMax Gold, Sigma) was administered five times (28-days-intervall). Antibodies were purified on an antigen-coupled CNBr-activated Sepharose® 4B column. The eluate was dialyzed against two changes of 5 l PBS for 24 h at 4°C, and finally concentrated to at least 1 μg IgG/μl.

Primary antibodies were diluted 1:100 in blocking buffer (PBS, 0.1% Triton-X100, 1% Tryptone/Peptone) and incubated for 60 min at RT. After washing in washing buffer (PBS, 0.05% Tween20, 0.3% Triton X100), sections were incubated for 1 h at RT in the dark with anti-rabbit atto647-conjugated secondary antibodies (Sigma-Aldrich, Cat. No. 40839) diluted 1:400 in blocking buffer. Sections were mounted onto microscope-slides and cover-slipped with Mowiol.

To analyze interaction of HA-5-HT1A and 5-ht5bmCherry in N1E-115 neuroblastoma cells, double-transfected live cells were first stained at low temperatures with rabbit-anti-HA-tag primary antibodies for 5 min and anti-rabbit atto647-conjugated secondary antibodies for 5 min to avoid internalization. Cells were then fixed and permeabilized before they were stained again with mouse anti-HA-tag primary antibodies and anti-mouse atto488-conjugated secondary antibodies.

Counterstaining of Intracellular Compartments

The plasmids to fluorescently label the cell membrane (pYFP-Mem), the ER (pYFP-ER), mitochondria (pYFP-mito) and peroxisomes (pEGFP-Pex) were obtained from Clontech. The plasmid to label the endosomes (GFP-Rab5; Addgene plasmid # 31733) was a gift from Richard Pagano (Choudhury et al., 2002). Lysosomes were counterstained with Lamp1-GFP.

Co-localization was observed using Zeiss LSM 510 Meta system. Quantitative analysis of co-localization was carried out by calculating Pearson’s correlation coefficients using LSM 510 software.

Confocal Laser-Scanning Microscopy

Distribution of recombinant receptors, organelle markers and immuno-fluorescent staining was analyzed by microscopy using a confocal laser scanning microscope LSM 510 Meta (Carl Zeiss, Jena, Germany) equipped with a 63× plan-apochromatic phase-contrast water-immersion objective, NA 1.4. Fluorophores were excited either with light at 458 nm, 488 nm or 514 nm from an Argon laser, at 543 nm from a HeNe laser or at 633 nm from a second HeNe laser. Emission of the fluorophores was recorded using the Meta detector. Analysis, e.g., intensity measurements, were performed by importing the images into ImageJ (Schneider et al., 2012). For plate assembly, images were digitally adjusted for brightness and contrast if necessary.

Förster Resonance Energy Transfer (FRET) Acceptor Photobleaching

Cells were transfected with equimolar amounts of 5-HT1A-GFP and 5-ht5b-mCherry or with GFP-rab5 and mRFP-rab5 (a gift from Ari Helenius (Addgene plasmid # 14437, Vonderheit and Helenius, 2005) or with single plasmids for negative control and fixed using 2% paraformaldehyde for 20 min prior to imaging. After collecting three images in both the GFP and the mRFP channels, the mRFP in the regions of interests (ROIs) were photobleached by scanning 50 times at high laser power. After photobleaching, again three images of both channels were taken. The obtained images were averaged to calculate the GFPbefore, GFPafter, mRFPbefore and mRFPafter values. The apparent Förster Resonance Energy Transfer (FRET) efficiency was calculated using the following formula: Apparent FRET efficiency = ((GFPafter − GFPbefore) × mRFPbefore) × ((GFPafter × mRFPbefore) − (GFPbefore × mRFPafter))−1 (van Royen et al., 2009). Image analysis was performed in ImageJ (Schneider et al., 2012).

Fluorescence Activated Cell Sorting (FACS) Analysis

To determine to what extent 5-ht5b expression affects translocation of 5-HT1A to intracellular organelles, we performed QD-mediated fluorescence activated cell sorting (FACS) analysis to measure the amount of surface expression of HA-5-HT1A. Cells expressing HA-5-HT1A and 5-ht5b at equimolar ratios were compared to cells expressing HA-5-HT1A transfected with the same amount of DNA together with an equimolar amount of unspecific cDNA to compensate for transcriptional effects. Cells were fixed in 2% paraformaldehyde/PBS for 15 min and labeled with excess of primary antibody against rabbit-anti-HA-tag (Santa Cruz, sc-805) and with a secondary antibody coupled to quantum dots (655 nm, Invitrogen). Avoiding cell permeabilization as well as the bulk of the QDs ensured that no intracellular proteins were labeled. Samples were run on a modified LSR II instrument from Becton and Dickinson using 405 nm excitation and a 660/40 nm emission filter.

Quantification of cAMP Signaling

The ability of 5-HT to modulate cAMP levels in cells under pharmacological treatment was assessed with the cAMP-Glo assay (Promega) according to the manufacturer’s instructions. cAMP amounts were determined by fitting the results from triplicate experiments to the standard curve. The phosphodiesterase inhibitor IBMX (50 mM) was present during this treatment.

Statistical Analysis

Statistical significance of the data was tested by one-way-ANOVA with Bonferroni’s post-test for multiple comparisons using GraphPad Prism 6 (GraphPad Software Inc., La Jolla, CA, USA) on a Microsoft Windows PC. A p-value of less than 0.05 was considered significant. Data are presented as mean ± standard error of the mean (SEM).

Results

The 5-ht5b Receptor Shows an Unusual Intracellular Localization

When expressed in N1E-115 cells, most 5-HT receptors produced a clear membrane-localized signal with minor staining of the Golgi apparatus due to trafficking (Figure 1A). With 5-HT4 and 5-HT6, membrane staining was strong, however a moderate amount of punctate clusters were visible in transfected cells. Only 5-ht5a and 5-ht5b showed a strong, punctate intracellular localization with little (5-ht5a) or no (5-ht5b) membrane staining at all. We have previously described that 5-ht5b is retained in intracellular organelles with the most significant co-localization found with endosomes and fluorescence immunohistochemistry on mouse brainstem sections detected 5-ht5b positive cells (Figure 1B01). High magnification images of this area revealed a clustered sub-cellular localization for 5-ht5b in these cells (Figures 1B02,03). 5-ht5b shows massive dysregulation in a mouse model of RTT (Vogelgesang et al., 2017). To follow up on the previously published results, we tested the sub-cellular localization of 5-ht5b in primary hippocampal neurons (Figure 1C) and could verify the results from N1E-115 cells with the highest co-localization of 5-ht5b with endosomal marker rab5 (0.867 ± 0.016), while markers for membrane (0.035 ± 0.007), mitochondria (0.538 ± 0.06), ER (0.273 ± 0.17) and lysosome (0.471 ± 0.11) showed little overlap.

FIGURE 1
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Figure 1. Subcellular localization of serotonin (5-HT) receptors in vitro and in vivo. (A) When expressed recombinantly in N1E-115 cells, 5-HT1A/2C/4/6/7 produce a clear membrane staining. In contrast, 5-ht5a/5b produce a distinct intracellular staining with weak (5-ht5a) or no (5-ht5b) membrane staining. Artificially truncating the other 5-HT receptors (here shown exemplarily for 5-HT7) produces the same intracellular pattern observed for 5-ht5a/5b. Scale bars represent 10 μm. (B) The intracellular localization of 5-ht5b is not an artifact of recombinant expression, but can be visualized in vivo. Immunohistological staining of murine brainstem (01) from hemizygous Mecp+/− mice against 5-ht5b (see “Materials and Methods” Section) reveals upon magnification (02) the same clustered intracellular localization (03) as seen in cells. Scale bars as indicated. Bregma is ~ −6.5. Abbreviations: Amb, Nucleus ambiguus; IOPr, inferior olive, principal nucleus; Sp5, spinal trigeminal tract. (C) Co-localization of 5-HT receptor 5-ht5b (purple) with cellular compartment markers (green) in primary hippocampal neurons. Neurons between DIV 9 to DIV 11 were transfected with fluorescently labeled 5-HT receptor 5-ht5b and compartment markers for membrane (GAP-43), endoplasmic reticulum (ER; recognition sequence of calreticulin), mitochondria (recognition sequence of cytochrome C-oxidase), lysosomes (Lamp-1) and endosomes (rab5). The strongest co-localization is with the endosomal marker. Scale bars in all images are 20 μm.

N-Terminal Glycosylation of 5-ht5 Receptors Controls Intracellular Localization

Based on literature and the truncation experiments, the most likely mechanism responsible for sorting proteins between membrane and intracellular organelles other than distinct localization signals is glycosylation of the N-terminus (Vagin et al., 2009; Guangyu, 2015). An influence of glycosylation on the trafficking of 5-ht5a was also shown previously (Dutton et al., 2008), with two glycosylation sites identified at N6 and N21 (Figure 2B). Incidentally, the intracellular clusters of 5-ht5a also co-localize strongest with endosomal markers (data not shown). Analyzing the protein sequences of 5-HT receptors, we found that strictly plasma membrane localized 5-HT1A receptor possess four N-terminal glycosylation sites (Figure 2A) at positions N10, N11, N24 and N30, while 5-ht5b receptors (Figure 2C) possess only one glycosylation site at position N5. As 5-ht5b can be detected in Western blots of murine brain both as a full length as well as a truncated protein (Vogelgesang et al., 2017), we tested if the truncation causes intracellular localization. An artificially truncated 5-HT7-trunc produced a similar staining with completely absent membrane localization and fluorescence concentrated in intracellular organelles (Figure 2D). However, 5-HT7-trunc co-localized strongest with the lysosomal marker (data not shown). Thus, the artificial truncation led to a defective receptor that either folds incorrectly or is otherwise marked for degradation and is sent to the lysosome.

FIGURE 2
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Figure 2. Effect of N-terminal glycosylation on membrane trafficking of 5-HT receptors. For all experiments, N1E-115 cells were transiently transfected with the same amount of receptor corresponding deoxyribonucleic acid (cDNA). All receptor constructs are shown in purple. If the outline of the cell was not easily recognized, a membrane label (GAP-43) was co-transfected (green). (A) 5-HT1A possesses four glycosylation sites on the N-terminus and displays specific membrane localization. (B) 5-ht5a possesses only two glycosylation sites. In comparison to the other 5-HT receptors, 5-ht5a shows weak membrane staining, but pronounced staining of endosomal compartments. (C) 5-ht5b possesses only one glycosylation site and membrane localization of the receptor is not detectable. (D) Artificially truncated 5-HT receptor 5-HT7 (5-HT7-trunc) comprises the trans-membrane domains (TMDs) IV to VII and shows strong intracellular clustering with no discernable membrane staining. (E) Site-directed mutagenesis of Asparagine (N) to Serine (S) at positions 24 and 30 in 5-HT1A-N24/30S removes two of four glycosylation sites and greatly reduces membrane trafficking of the mutated receptor. (F) Tunicamycin blocks the formation of protein N-glycosidic linkages by inhibiting the transfer of N-acetylglycosamine-1-phosphate to dilichol mono-phosphate. Application of Tunicamycin (1 μg/ml) to cells expressing 5-HT1A removes the receptor from the cell membrane. (G) Replacing the N-terminal domain of 5-HT1A containing 4 glycosylation sites with the N-terminal domain of 5-ht5b with 1 glycosylation site completely abolishes membrane localization of the hybrid receptor and produces a clustered intracellular staining. (H) Replacing the N-terminal domain of 5-ht5b containing 1 glycosylation site with the N-terminal domain of 5-ht5a with 2 glycosylation sites produces a clustered intracellular staining and produces moderate membrane localization. (I) Replacing the N-terminal domain of 5-ht5b containing 1 glycosylation site with the N-terminal domain of 5-HT1A with 4 glycosylation sites does not prevent intracellular localization, but leads to significant membrane localization of the hybrid receptor. Scale bars in all images are 10 μm.

In contrast, the number of glycosylation sites corresponds well with the strength of membrane expression with no discernable membrane staining in case of 5-ht5b (Figure 2C), weak staining for 5-ht5a (Figure 2B) and strong staining for 5-HT1A (Figure 2A).

Successive removal of glycosylation sites in 5-HT1A by site-directed mutagenesis led to increasing loss of surface expression. While removing one glycosylation site had no visible effect (data not shown), removal of two glycosylation sites produced only weak surface expression and strong endosomal accumulation of the receptor (Figure 2E). Removal of three or more glycosylation sites led to a total loss of surface expression (data not shown). Complete, yet unspecific de-glycosylation of 5-HT1A receptors with 1 μM Tunicamycin (Figure 2F) blocked cell surface localization of the receptor indicating a glycosylation dependence of its trafficking.

Hybrid receptor constructs composed of the extracellular N-terminus of 5-HT1A or 5-ht5a receptors and the 5-ht5b receptor (Figures 2H,I) reconstitute 5-ht5b receptor localization on the cell membrane with staining intensity depending on the strength of the glycosylation signal. In contrast, fusion of the N-terminus of 5-ht5b to 5-HT1A abolishes membrane localization (Figure 2G). As it had already been confirmed for 5-ht5a (Dutton et al., 2008), we concluded that N-terminal glycosylation also determines the membrane trafficking of 5-ht5b.

5-ht5b Specifically Interacts with 5-HT1A

Knowing that many GPCRs (Gurevich and Gurevich, 2008; Schwenk et al., 2010) and some 5-HT receptors in particular (Pellissier et al., 2011; Renner et al., 2012) form homo- or heterodimers, we wanted to know whether co-expression with other 5-HT receptors could lead to a stronger surface expression of 5-ht5b.

We co-expressed a representative member of each 5-HT receptor subgroup tagged with mCherry against the same set of 5-HT receptors now tagged with GFP (Figure 3A). However, we excluded 5-HT3R in this matrix because it is a multimeric ion channel (Uetz et al., 1994; Boyd et al., 2002). Quantification of the correlation coefficients revealed three separate populations (Figure 3B). Here, one population corresponds to the receptor pairs that co-localize to the plasma membrane while the other corresponds to receptor pairs that remain separated between membrane and intracellular organelles. The third population was comprised of the receptor pairs that showed possible interaction. Of this group, the receptor pair of 5-HT1A and 5-ht5b displayed the most unusual behavior, with 5-ht5b not showing enhanced surface expression, but instead retaining 5-HT1A in the endosomal compartments with select specificity (Figure 3A04). This change of 5-HT1A’s sub-cellular localization could also be reproduced in primary neurons (Figure 3C).

FIGURE 3
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Figure 3. 5-ht5b specifically interacts with 5-HT1A to change the latter’s subcellular localization. (A) We transfected a representative member of each 5-HT receptor subgroup tagged with mCherry against the same set of 5-HT receptors tagged with GFP. Each image of the matrix shows N1E-115 cells co-expressing two 5-HT receptors. The images are pseudo-colored purple for the receptor indicated horizontally and pseudo-colored green for the receptor indicated vertically. Co-localization is shown in yellow. 5-ht5b specifically interacts with 5-HT1A (04) with the normally strictly membrane-bound 5-HT1A receptors partly retained intracellularly. In addition, 5-ht5a seems to interact with 5-HT4 (12) and 5-HT6 seems to weakly interact with 5-ht5a (17) and 5-ht5b (19), although 5-HT6’s surface expression remains strong. No other 5-HT receptors seem to interact with each other in a way that changes subcellular localization. Scale bars in all images are 10 μm. (B) For quantification, we separately calculated Pearson’s correlation coefficients for the fluorescence signals at the membrane and at intracellular organelles by manually applying regions of interest (ROI). Plotting the organelle correlation coefficient over the membrane correlation coefficient for each receptor pair resulted in three populations of receptors. One population displays a high correlation at the membrane, but not at intracellular organelles. The second population displays correlation in neither compartment while the third population displays high correlation at intracellular compartments. (C) To verify interaction of 5-HT1A and 5-ht5b, we transfected primary hippocampal neurons with expression constructs of both receptors. 5-HT1A (green) localizes to the cell membrane, while 5-ht5b (purple) localizes to intracellular organelles, while co-expression of both receptors shows intracellular co-localization with no discernable membrane staining by 5-HT1A. Scale bars in all images are 20 μm.

After observing the retention of 5-HT1A on intracellular organelles by 5-ht5b, we looked for the mechanism. With GPCRs known to form oligomers, direct interaction was an obvious answer, but overloading of the transport pathway was also possible. To differentiate between both mechanisms, we performed a series of experiments while always using equal amounts of transfected DNA.

An early indicator for interaction was the specificity of interaction. The change of subcellular localization only happens between 5-HT1A and 5-ht5b, but not between 5-HT1A and any other receptor or 5-ht5b and any other receptor.

First, we tested direct interaction using acceptor-photobleaching FRET (abFRET) microscopy (Figure 4A) using GFP- and mRFP-labeled constructs (see Materials for details). Apparent FRET efficiency (Fapp) of the two 5-HT receptors was 29.74% ± 1.6, which was even slightly higher than two rab5’s expressed together (25.58% ± 4.6). Here, a strong FRET signal is expected as the proteins localize to the same organelles and are therefore in close proximity. Testing unspecific interaction by co-expressing 5-ht5b with rab5 showed a significantly lower Fapp of 9.56% ± 1.1. Here, some FRET might be expected, as 5-ht5b co-localizes with endosomes (Figure 1C), but the FRET signal was significantly smaller compared to the 5-HT1A:5-ht5b signal. The protein pair of 5-ht5b and Lamp1 produced a very low Fapp of 0.02% ± 0.7, as the proteins are on separate organelles (Vogelgesang et al., 2017) and only interact very little.

FIGURE 4
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Figure 4. Analysis of receptor interaction. (A) Acceptor-photobleaching Förster Resonance Energy Transfer (abFRET) microscopy was used to determine the extent of protein:protein-interaction. Protein pairs of 5-HT1A:5-ht5b, rab5:rab5, 5-ht5b:rab5 and 5-ht5b:Lamp1 were co-expressed in N1E-115 cells at equimolar concentrations and the apparent FRET efficiency (Fapp) was measured. The color-coded image shows an exemplary experiment of 5-HT1A:5-ht5b, while the bar diagram shows the apparent FRET efficiencies of 5-HT1A:5-ht5b (29.74 ± 1.6), rab5:rab5 (25.58 ± 4.6), 5-ht5b:rab5 (9.56 ± 1.1) and 5-ht5b:Lamp1 (0.02 ± 0.7). Asterisks indicate significance (***p ≤ 0.001; one-way-ANOVA with Bonferroni’s post-test for multiple comparisons). (B) Immunohistochemical analysis of distribution and equal expression levels. Non-permeabilized cells were stained for 5-HT1A (green), then fixed and permeabilized and stained again for 5-HT1A (purple). 5-ht5b is co-expressed in some cells as a fusion protein with a fluorescent tag (red). The fluorescence intensity of the first 5-HT1A staining was then measured in cells expressing 5-HT1A and in cells expressing 5-HT1A and 5-ht5b. The cartoon shows the experimental procedure. The bar diagram shows the mean fluorescence intensities of 5-HT1A reactivity in cells expressing only 5-HT1A and in cells expressing 5-HT1A (1.0 ± 0.06) and 5-ht5b (0.52 ± 0.08) (***p ≤ 0.001; unpaired t-test). (C) The effect of 5-HT1A:5-ht5b co-expression on 5-HT1A surface localization was quantified by fluorescence activated cell sorting (FACS) analysis of N1E-115 cells expressing HA-5-HT1A alone or together with 5-ht5b. Expressing 5-HT1A together with an equal amount of filler DNA was used to determine 5-HT1A surface expression under control conditions (blue). Co-expression of 5-HT1A with an equal amount of non-interacting 5-ht5a did not change the degree of surface expression (green). Co-expression of 5-HT1A with an equal amount of 5-ht5b decreased the cell surface expression of 5-HT1A by 48.8% ± 17.4%. The cartoon shows the experimental procedure. Labeling was directed at HA-tag on 5-HT1A with quantum dot-coupled secondary antibodies. To avoid skewing results by transcription level effects in the control measurement, an unspecific filler plasmid (mock) was co-transfected in place of the second receptor to maintain the same total amount of transfected plasmid.

Then, to quantify the surface expression of 5-HT1A in the absence and in the presence of 5-ht5b, we used fluorescence microcopy (Figure 4B). First, we stained only surface-expressed 5-HT1A (green) in live cells, as antibodies cannot penetrate through the membrane. Then we fixed and permeabilized the cells and stained 5-HT1A again with different primary and secondary antibodies, this time staining both surface-expressed as well as internal receptors (purple). Cells co-expressing 5-ht5b were identified by its inherent mCherry-fusion fluorescent signal (red). We quantified the fluorescence intensity of surface-expressed 5-HT1A (green) in cells with and without 5-ht5b signal and found a reduction of 5-HT1A surface expression by 52.3% ± 8.05 in cells co-expressing 5-ht5b.

To quantify 5-HT1A in a larger amount of cells, we used FACS (Figure 4C). Cells expressing 5-HT1A together with an equal amount of filler DNA was used to determine 5-HT1A surface expression under control conditions. Co-expression of 5-HT1A with an equal amount of 5-ht5a did not change the degree of surface expression. This indicates that the mere presence of another plasmid or receptor did not affect the membrane localization of 5-HT1A. However, the surface expression of 5-HT1A was reduced by 48.8% ± 17.4% when it was expressed with an equal amount of 5-ht5b (Figure 4C). The reduction of surface-expressed 5-HT1A was consistent with the reduction seen with immunohistochemistry (Figure 4B).

While the translocation of 5-HT1A to a different sub-cellular localization was obvious (Figure 3A04), the amount of surface availability could also be affected by different expression levels caused through co-transfection. As expression of all receptor constructs is CMV driven and all construct have roughly the same size, we regard this as unlikely. Nevertheless, we analyzed whether expression levels of 5-HT1A were affected by co-transfection by comparing the fluorescence intensity of 5-HT1A-GFP in cells expressing equal amounts of 5-HT1A and a filler DNA or cells expressing 5-HT1A and 5-ht5b. Although expression levels of both receptors fluctuated in individual cells, we found no significant overall differences (Supplementary Figure S1) that could explain the 2-fold reduction in surface expression seen above.

With direct interaction being the most likely mechanism, we cannot rule out indirect interaction. It has been shown previously that transport of 5-HT1A in neurons is controlled by co-factor Yif1b (Carrel et al., 2008), but the involvement of adaptor proteins will be the topic of further studies.

While the change in subcellular localization was most pronounced for 5-HT1A by 5-ht5b, for completeness we would like to mention additional possible interactions that were revealed by plotting the correlation coefficients (Figure 3B). We found that 5-ht5a co-localized with 5-HT4 (Figure 3A12) and that both 5-ht5 receptors showed moderate co-localization with 5-HT6 (Figures 3A17 and 3A19). Although intracellular aggregation became more pronounced upon co-expression, both 5-HT4 and 5-HT6 showed already minor intracellular clusters when expressed alone (Figure 1A). In these cases, overloaded trafficking is a more likely mechanism, but analysis is more complicated and will be done at a later time.

Co-Expression of Serotonin Receptors in the Mouse Brain

We used RT-PCR to determine the expression of all receptors in different regions of the brain (Figure 5). RT-PCR confirmed wide-spread 5-HT receptor expression in the murine brain with multiple receptors being expressed in basically every region analyzed. Among these, the hippocampal formation showed the largest diversity of all regions analyzed. Specifically, for 5-HT1A and 5-ht5b, we found regional co-expression in the bulbus olfactorius, the hippocampal formation and the brainstem.

FIGURE 5
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Figure 5. Expression of 5-HT receptors in the mouse brain. RT-PCR was used to detect expression of all 5-HT receptors in select brain regions of mice. CTX, cortex; OLF, bulbus olfactorius; HFP, hippocampal formation; MB, midbrain; CB, cerebellum; BS, brainstem.

Identification of Interaction Domains

Having prepared some hybrid receptors for the study of glycosylation and trafficking, we continued this strategy to try and define domains which would explain the specific interaction between 5-HT1A and 5-ht5b (Figure 6A).

FIGURE 6
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Figure 6. Identification of possible interaction domains between 5-HT1A (green) and 5-ht5b (purple). N1E-115 cells were transiently transfected with two hybrid receptor variants labeled with eGFP or mCherry. (A) Co-expression of full length 5-HT1A and full length 5-ht5b lead to strong internalization of 5-HT1A. (B) Replacing the C-terminal domain of 5-ht5b with the C-terminal domain of 5-HT1A (HRV-15) did not change the amount of interaction. (C) Expressing 5-HT1A together with a hybrid 5-HT1A where the 3rd intracellular loop and the last two TMDs are from 5-ht5b (HRV-17), the interaction is greatly reduced or even abolished. (D) Expressing 5-HT1A together with a hybrid receptor composed of the first three TMDs of 5-HT1A and the last four TMDs of 5-ht5b (HRV-18) show interaction as the two full length receptors.

Replacing the PDZ-like C-terminal domain of 5-ht5b with that of 5-HT1A had no influence on subcellular localization or interaction (HRV-15, Figure 6B).

A hybrid receptor (HRV-17) consisting of 5-HT1A (from start up to TMD V) and 5-ht5b (intracellular loop 3 (ICL3) and onwards) can interact with wild type 5-HT1A, although not as strong as seen between both wild-type receptors. This indicated that ICL3 contains at least parts of the interaction domain (Figure 6C).

Exchanging TMD IV and V of 5-HT1A in the previous hybrid clone by TMD IV and TMD V of 5-ht5b, thus creating HRV-18, fully restored the interaction to levels seen for the wild-type receptors (Figure 6D).

Physiological Consequences of 5-ht5b Expression

The strong and far-ranging expression of 5-ht5b (Figure 5) indicates some physiological significance. However, given its intracellular expression, 5-ht5b differs from classical GPCRs. With at best sparse surface expression, 5-ht5b seems to contribute little to intracellular signaling. However, a more likely function of 5-ht5b could be the modulation of its interaction partner by affecting its surface availability.

The strictly intracellular 5-ht5b did not respond to stimulation by 5-HT (−9.46% ± 1.296, Figure 7II), however, the mere presence of 5-ht5b decreased the cAMP level, indicating some constitutive activity of 5-ht5b (−7.75% ± 1.012, Figure 7I). For 5-HT1A no constitutive activity was measurable (−2.49% ± 1.366, Figure 7III), while application of 5-HT decreased cAMP (−28.12% ± 1.096, Figure 7IV). Cells transfected with both receptors showed reduced cAMP levels (−10.37% ± 1.029, Figure 7V). Application of 5-HT to cells co-expressing both receptors produced a reduction of cAMP (−19.91% ± 2.219, Figure 7VI), as activation of 5-HT1A decreased cAMP despite the reduced baseline cAMP level due to 5-ht5b’s constitutive activity. The reduction of cAMP was smaller compared to cells expressing 5-HT1A alone, yet significant (p = 0.002). This clearly showed that co-expression of 5-ht5b can affect the signaling behavior of other 5-HT receptors.

FIGURE 7
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Figure 7. Physiological consequences of 5-HT1A:5-ht5b co-expression. To test whether translocation of 5-HT1A by 5-ht5b effects cyclic adenosine monophosphate (cAMP) signaling, we measured the cellular cAMP level under various conditions. To measure the decrease of cAMP, 50 nM Forskolin was added to all cells before the start the experiment to increase cAMP levels. Mock-transfected cells treated with Forskolin and stimulated with 1 μM 5-HT served as control and were set to 100%. In all experiments, cells were transfected with an equimolar amount of DNA. To keep the amount of DNA the same in experiments with only one receptor, a filler plasmid was co-transfected. Expression of 5-ht5b without stimulation with 5-HT decreased cAMP by −7.75% ± 1.012 (I), while addition of 5-HT did not enhance the reaction (−9.46% ± 1.296; II). Expressing 5-HT1A in cells had no effect on cAMP levels without stimulation (−2.49% ± 1.366; III), but adding 5-HT decreased cAMP by −28.12% ± 1.096 (IV). Co-expression of 5-HT1A and 5-ht5b together without stimulation by 5-HT lead to a drop in cAMP by −10.37% ± 1.029 (V). Adding 5-HT to co-expressing cells dropped the cAMP level by −19.91% ± 2.219 (VI). Asterisks indicate significance (**p ≤ 0.01; ***p ≤ 0.001; one-way-ANOVA with Bonferroni’s post-test for multiple comparisons).

Discussion

In this study we described the behavior of 5-HT receptor 5-ht5b, which manifests in intracellular localization to endosomal compartments and specific interaction with another select member of the 5-HT receptor family.

5-ht5b localizes to endosomes (Figure 1C), which was also seen for 5-ht5a (data not shown) and therefore might present a defining feature of this sub-group of 5-HT receptors. It might also indicate a physiological significance, as other truncated receptors are retained mainly in the ER (Karpa et al., 2000; Leung et al., 2007; Gonzalez et al., 2011). It is known that many GPCRs naturally show constitutive activity or that constitutively active mutants exist (Tao, 2008). GPCRs were even described to signal from endosomal vesicles after internalization (Irannejad et al., 2013). Internal signaling might be indicated by the fact that we could measure a minor decrease of cAMP upon expression of 5-ht5b without application of a ligand (Figure 7).

In the literature, several mechanisms, including glycosylation (Dutton et al., 2008), TMD size (Sharpe et al., 2010) or N-terminal signal peptides (Jahnsen and Uhlen, 2012) are discussed to control receptor trafficking to the membrane. The unusual intracellular localization of 5-ht5a and 5-ht5b seems to be caused in large part by glycosylation of the N-terminus as artificially increasing the number of glycosylation sites of 5-ht5b increases its surface localization (Figures 2H,I). This form of glycosylation was also found to control membrane localization of 5-ht5a (Dutton et al., 2008).

Formation of hetero-oligomers has been described for many GPCRs (Schwenk et al., 2010) including 5-HT receptors (Pellissier et al., 2011; Renner et al., 2012), although their interaction is subtle and its physiological significance remains to be shown. Here, 5-ht5b‘s affinity to 5-HT1A was so strong that it changes the subcellular localization of 5-HT1A. As both 5-HT receptors were found co-expressed in the brain (Figure 5), it is feasible to assume a physiological role for this specific interaction. The interaction mapping is still only rudimentary, but efforts to identify the binding interfaces of class A GPCRs have been ongoing for years, with most studies leaning towards TMD IV and TMD V as dimerization interface (González-Maeso et al., 2008; Johnston et al., 2011; Hu et al., 2012). These were also identified here as a possible location for the interaction interface. With the strong interaction between 5-HT1A and 5-ht5b and an easy read-out through translocation, further studies to fine-map the interaction surface might profit.

The mostly intracellular 5-ht5b receptor probably does not relay signals in the conventional way, but by retaining 5-HT1A in intracellular compartments, 5-ht5b reduces its surface expression significantly, thus effectively reducing 5-HT1A’s contributions to cellular signaling (Figures 4, 7). In alternate modes of action, 5-ht5b might modify intracellular signaling by acting on the cAMP level, either through constitutive activity and/or by scavenging G-proteins which would no longer be available for other signal cascades.

It is difficult to define a role for the 5-HT1A:5-ht5b interaction in RTT, as the syndrome displays very complex genetic imbalances and many different and sometimes opposing therapies seem to improve symptoms in RTT. Within the serotonergic system alone, two previous observations in animal models of RTT might be linked to 5-HT1A:5-ht5b. Application of 5-HT1A agonists was described to have beneficial effects on the respiratory phenotype in mice (Abdala et al., 2010) and might be linked to the reduction of surface-expressed 5-HT1A by 5-ht5b. In contrast, treatment with 5-HT7 agonists was reported to improve behavior (De Filippis et al., 2014, 2015a) and might counteract the constitutive down-regulation of cAMP by 5-ht5b.

However, we would like to advise some caution interpreting these results. Here, we transfected recombinant cDNA at equimolar concentrations into cell lines and measured the effect of receptor activation on cAMP. In vivo, the situation is most likely much more complicated, as receptor expression levels may not be equal, co-factors might be present and signaling cascades are more complex. For example, we did not measure effects on CNG ion channels or on small GTPases. Of interest regarding the physiological function of 5-ht5b is the fact that 5-HT1A also becomes internalized upon activation, after which it seems to activate the Erk-1/2 signaling pathway (Renner et al., 2012). This is especially interesting as 5-ht5b initially came to our attention when analyzing a mouse model of RTT (Vogelgesang et al., 2017) and modulation of small RhoGTPase activity was shown to have beneficial effects on RTT (De Filippis et al., 2012, 2015b).

Author Contributions

SN, GJB, SV, TM and MN performed experiments. SN and MN wrote the manuscript.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

This work was supported by the Cluster of Excellence and Deutsche Forschungsgemeinschaft (DFG) Research Center Nanoscale Microscopy and Molecular Physiology of the Brain. We acknowledge support by the Open Access Publication Funds of the Göttingen University. We would like to thank Christina Schäfer for the preparation of primary hippocampal neurons and Prof. Swen Hülsmann for helpful discussions.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/article/10.3389/fnmol.2017.00299/full#supplementary-material

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Keywords: 5-ht5b receptor, 5-HT1A receptor, Rett syndrome, signaling, cAMP

Citation: Niebert S, van Belle GJ, Vogelgesang S, Manzke T and Niebert M (2017) The Serotonin Receptor Subtype 5b Specifically Interacts with Serotonin Receptor Subtype 1A. Front. Mol. Neurosci. 10:299. doi: 10.3389/fnmol.2017.00299

Received: 20 June 2017; Accepted: 06 September 2017;
Published: 21 September 2017.

Edited by:

Rameshwar K. Sharma, Salus University, United States

Reviewed by:

Pere Garriga, Universitat Politecnica de Catalunya, Spain
Martin Heine, Leibniz Institute for Neurobiology, Germany

Copyright © 2017 Niebert, van Belle, Vogelgesang, Manzke and Niebert. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Marcus Niebert, mnieber@gwdg.de