Kainate receptors are key modulators of synaptic transmission and plasticity in the central nervous system. Different kainate receptor isoforms with distinct spatiotemporal expression have been identified in the brain. The GluK1-1 splice variant receptors, which are abundant in the adult brain, have extra fifteen amino acids inserted in the amino-terminal domain (ATD) of the receptor resulting from alternative splicing of exon 9. However, the functional implications of this post-transcriptional modification are not yet clear. We employed a multi-pronged approach using cryogenic electron microscopy, electrophysiology, and other biophysical and biochemical tools to understand the structural and functional impact of this splice insert in the extracellular domain of GluK1 receptors. Our study reveals that the splice insert alters the key gating properties of GluK1 receptors and their modulation by the cognate auxiliary Neuropilin and tolloid-like (Neto) proteins 1 and 2. Mutational analysis identified the role of key splice residues that influence receptor properties and their modulation. Furthermore, cryoEM structure of the variant shows that the presence of exon 9 in GluK1 does not affect the receptor architecture or domain arrangement in the desensitized state. Our study thus provides the first detailed structural and functional characterization of GluK1-1a receptors, highlighting the role of the splice insert in modulating receptor properties and their modulation.
This important study shows that a splice variant of the kainate receptor Glu1-1a that inserts 15 amino acids in the extracellular N-terminal region substantially changes the channel's desensitization properties, the sensitivity to glutamate and kainate, and the effects of modulatory Neto proteins. The functional data supporting the role of the 15 amino acid insert are solid, although some clarifications and more data are needed to determine the molecular mechanism by which the insert changes the functional profile of the channel. Even so, these findings substantially advance our understanding of splice variants among glutamate receptors and will be of interest to neuro- and cell-biologists and biophysicists in the field.
Kainate receptors (KARs), a subfamily of ionotropic glutamate receptors (iGluRs), are required in the vertebrate brain for postsynaptic neurotransmission and presynaptic regulation of transmitter release (Erreger et al., 2004; Huettner, 2003; Lerma, 2003; Pinheiro and Mulle, 2006). They are known to mediate characteristic small-amplitude excitatory postsynaptic currents (EPSC) with slow kinetics in the hippocampal regions of the central nervous system compared to their counterparts, α-amino-3-hydroxy-5-methyl-4-isoxazole propionic acid (AMPA) and N-methyl-D-aspartate (NMDA) receptors (Castillo et al., 1997; Lerma et al., 2001; Traynelis et al., 2010). Furthermore, they play a vital role in the maturation of neuronal circuits during development by interacting with G proteins (Lerma, 2003; Lerma and Marques, 2013). Any functional defect predisposes the brain to various disorders such as autism, epilepsy, schizophrenia, and neuropathic pain (Lerma and Marques, 2013; Bowie, 2008; Valbuena and Lerma, 2021).
Kainate receptors are composed of subunits from two gene families: low kainate affinity and high kainate affinity. The first gene family includes GluK1-GluK3, which can form both homomeric and heteromeric receptors with subunits from the same family or from the high-kainate affinity family. On the other hand, GluK4-GluK5 are high-affinity subunits that must assemble with low-affinity subunits in order to create functional receptors. The assembly of different subunits results in the formation of various receptor configurations, which contribute to the wide range of functional properties observed in kainate receptors.
The functional repertoire of kainate receptors is further enhanced by RNA editing (Barbon and Barlati, 2011; Seeburg, 2002) and alternative splicing (Jaskolski et al., 2004). In particular, GluK1-containing KARs that are mainly present in the hippocampus, cortical interneurons, Purkinje cells, and sensory neurons, undergo alternative splicing and RNA editing (Bernard and Khrestchatisky, 1994). Alternative splicing of the C-terminal domain that produces four isoforms, GluK1-a (shortest C-terminal), GluK1-b, GluK1-c, and GluK1-d (Bettler et al., 1990; Gregor et al., 1993; Pinheiro and Mulle, 2006; Sommer et al., 1992) has been studied (Ren et al., 2003). However, the functional impact of the mRNA splicing of the N-terminal domain (exon 9) resulting in isoforms GluK1-1 and GluK1-2, with GluK1-1 containing an additional 15 amino acids in the amino-terminal domain (ATD) is not understood. The splice junctions for GluK1-1 were reported to be more frequent than those for GluK1-2, and both variants showed similar expression in different species (Herbrechter et al., 2021). This 15-amino acid insertion in the amino-terminal domain (ATD) is exclusive to the GluK1 subunit and may impart unique properties to KARs containing this variant. Therefore, investigations of functional differences between GluK1 receptors with and without the 15 amino acid splice insert are necessary but missing in the field. Furthermore, the impact of the N-terminal splice insert in GluK1-1 receptors on its modulation by cognate auxiliary subunits (Fisher, 2015; He et al., 2021a; Sheng et al., 2015; Vinnakota et al., 2021), neuropilin and tolloid-like (Neto) proteins is also unknown.
Therefore, we conducted structure-function studies to understand the mechanisms of GluK1-1a receptor function and the effects of the ATD splice on receptor assembly, stability, and modulation by Neto proteins. Whole-cell and excised outside-out patch-clamp-based functional assays were performed to investigate the differences between the ATD splice variants GluK1-1a (exon 9) and GluK1-2a (lacking exon 9), and their modulation by Neto proteins. Furthermore, mutational analysis was performed to identify important splice residues that affect receptor functions and their modulation by Neto proteins. Additionally, we expressed and purified rat GluK1-1a from HEK293 GnTI-cells and determined the single-particle cryo-EM structures of the receptors trapped in the desensitized state to understand effect of splice on receptor architecture.
Spatiotemporal expression pattern of GluK1-1 in the brain
Kainate receptor subunits are differentially and spatially regulated in vertebrates. We analyzed publicly available human transcriptomic data to determine whether the exon encoding the GluK1 ATD splice (exon 9) was differentially expressed in the human brain. RNASeq data analysis of GRIK1 (Ensembl ID: ENSG00000171189) collected from BrainSpan ATLAS indicated that exon 9 is present in multiple areas of the brain that also show prominent GluK1 expression, such as the cerebellar cortex (Figure 1; Figure 1-figure supplement 1). Variable expression of exon 9 in different areas of the brain prompted us to delve deeper into the molecular mechanisms and perform a structure-function analysis of this GluK1 splice variant.
The ATD splice imparts functional diversity to GluK1 receptors
Previous studies on functional analysis of GluK1 receptors have primarily focused on GluK1-2 isoform that lacks the ATD splice insert. Therefore, we carried out extensive electrophysiological investigation to assay the functional differences between GluK1-1a and GluK1-2a. The only difference between these two variants is the presence of 15 amino acid (KASGEVSKHLYKVWK) insertion in the R2 subdomain (lower lobe) of the GluK1-1a ATD. We evaluated multiple gating properties of the two variants by whole-cell patch-clamp electrophysiology. Interestingly, we observed that GluK1-1a receptors desensitize significantly slowly when compared to GluK1-2a (ƮDes, GluK1-1a: 5.21 ± 0.50 ms; GluK1-2a: 3.55 ± 0.23 ms **P=0.0092) on prolonged treatment with 10 mM glutamate (Figure 2A; Table 1). We also tested receptor desensitization on application of saturating concentrations of kainate (1mM). Since the receptors displayed very slow desensitizing kainate currents, instead of the rate (ƮDes), we calculated the % desensitization values at 1 s for comparison. We observed that the % desensitization with kainate was distinct for both ATD splice variants with significantly slower desensitization in the variant with the splice insert (GluK1-1a: 72.06 ± 2.33 %, GluK1-2a: 93.2 ± 0.55 ***P=0.0006) consistent with the glutamate evoked currents (Figure 2B; Table 1).
Next, we evaluated glutamate sensitivity for the two variants. Dose-response experiments (glutamate, GluK1-1a: 0.1-2 mM, and GluK1-2a: 0.01-3 mM), showed a significantly lower potency of glutamate for GluK1-1a variant compared to the non-spliced form (EC50 glutamate, GluK1-1a: 379.3 ± 52 µM, GluK1-2a: 187.7 ± 33 µM *P=0.0129 (Figure 2C Table 1). However, for high-affinity agonist kainate, the dose-response curves for both variants were similar likely indicating differences in the stability of glutamate versus the kainate-bound states in GluK1-1a and GluK1-2a (Figure 2D; Figure 2-figure supplement 1). Thus, the potency of kainate (1mM) versus glutamate (10 mM) (IK/IG ratio) is significantly higher for GluK1-1a compared to GluK1-2a (GluK1-1a: 1.51 ± 0.13, GluK1-2a: 0.56 ± 0.4 ****P< 0.0001) (Figure 2D; Table 1).
Further, we investigated the voltage-dependent polyamine block and found significant differences between the two variants. The presence of splice residues seemed to enhance outward currents at positive potentials in GluK1-1a compared to GluK1-2a (rectification index, +90mV /-90 mV; GluK1-1a = 0.96 ± 0.11; GluK1-2a = 0.61 ± 0.10 *P=0.0385) without affecting the reversal potential (Figure 2E; Table 1). It’s unclear how splice residues situated ∼30 Å away from the TM domain affect the pore properties. This property is mainly affected by the TM2 region of the KAR (Bowie and Mayer, 1995), although a recent report in which the ATD of GluK2 was deleted showed enhanced rectification (Li et al., 2019). It’s likely that the presence of splice residues alters pore structure thereby affecting rectification (Perrais et al., 2009). We also carried out outside-out patch recordings to examine GluK1-1a receptors. However, we observed extremely weak electrical currents with low amplitudes when GluK1-1a was expressed in isolation. As a consequence, the data we obtained from these recordings did not provide reliable results for curve fitting or thorough analysis.
ATD splice insert impacts GluK1 receptor modulation by Neto proteins
Neto 1 and Neto 2 proteins significantly influence the surface expression, synaptic localization, and functional properties of the GluK1-2a receptors (Copits et al., 2011; Palacios-Filardo et al., 2016; Sheng et al., 2015). It has been demonstrated that desensitization of GluK1-2a is accelerated by Neto1 but delayed by Neto2 (Sheng et al., 2015; Copits et al., 2011; Palacios-Filardo et al., 2016). Hence, to understand the influence of these KAR auxiliary proteins on GluK1-1a, we performed an electrophysiological analysis of GluK1-1a and GluK1-2a receptors co-expressed with either Neto1 or Neto2. Co-expression of Neto1 hastened desensitization of GluK1-1a significantly but not of GluK1-2a at saturating glutamate concentrations (ƮDes, GluK1-1a +Neto1: 3.56 ± 0.22 ms **P=0.0090; GluK1-2a +Neto1: 4.32 ± 0.34 P=0.1495). On the other hand, Neto2 led to a ∼ 13.4-fold decrease in the desensitization rate of GluK1-1a (ƮDes, GluK1-1a: 5.21 ± 0.50 ms, +Neto2: 69.62 ± 9.98 ms **P=0.0024) while the desensitization rate of GluK1-2a was delayed only by ∼ 6.1-fold (ƮDes, GluK1-2a: 3.55 ± 0.23 ms, +Neto2: 21.68 ± 2.64 ms **P=0.0017). Thus, while Neto1 accelerated the desensitization of GluK1-1a, Neto2 significantly slowed it at saturating glutamate concentrations. When both GluK1-1a and GluK1-2a were coexpressed with Neto2, the rate of desensitization for GluK1-1a was approximately 3.2 times slower compared to GluK1-2a (***P=0.0009) (Figure 3A; Table 1. Thus, the presence of splice insert leads to differential modulation of GluK1 desensitization by Neto proteins.
Moreover, Neto1 also enhanced the recovery from desensitization for both the variants (ƮRecovery, GluK1-1a: 3.53 ± 0.81 s, +Neto1: 0.68 ± 0.07 s *P=0.0390; GluK1-2a: 5.31 ± 0.50 s +Neto1: 1.15 ± 0.12 s ***P=0.0002). GluK1-1a recovers ∼ 1.7 times faster than GluK1-2a (*P=0.0125) when co-expressed with Neto1. Neto 2, on the other hand, slowed recovery for both variants to a similar extent (ƮRecovery, GluK1-1a: 3.53 ± 0.81 s, +Neto2: 8.32 ± 0.81 s **P=0.0044; GluK1-2a: 5.31 ± 0.50 s, +Neto2: 7.91 ± 0.71 s *P=0.0430) and did not show differential modulation (Figure 3B; Table 1). In addition, both Neto1 and Neto2 increased the potency of glutamate for GluK1-1a by 9.7-fold (39 ± 10 µM) and 11.2-fold (34 ± 8 µM), respectively (Figure 3C; Figure 3-figure supplement 1A). This is similar to the effect observed in GluK1-2 receptors whereby the glutamate EC50 was shown to increase by Neto proteins [Neto1: 34-fold and Neto2: 7.5-fold (Palacios-Filardo et al., 2016) and Neto1/2: 10-30X (Fisher, 2015)].
Since we observed a significant increase in the IK/IG ratios in GluK1 due to the presence of splice insert, we next aimed to determine the influence of co-expressing Neto proteins on this parameter. Interestingly, we observed that while Neto 1 and Neto2 reduced the IK/IG ratios in GluK1-1a (GluK1-1a: 1.51 ± 0.13, +Neto1: 1.25 ± 0.04 P=0.1500, +Neto2: 1.0 ± 0.07 **P=0.0090), they increased it for the non-spliced variant (GluK1-2a: 0.56 ± 0.04, +Neto1: 1.37 ± 0.12 ****P<0.0001, +Neto2: 1.16 ± 0.04 ****P<0.0001) (Figure 3D; Figure 3-figure supplement 1B; Table 1) (Zhang et al., 2009) highlighting the effect of splice residues. Interestingly, this differential modulation of the two variants by Neto proteins resulted in comparable IK/IG ratios.
Next, we investigated the effects of Neto1 and Neto2 on the voltage dependent endogenous polyamine block since presence of splice insert had enhanced the outward rectification of GluK1. We observed that both Neto1 and Neto2 significantly enhanced the outward rectification of GluK1-2a (GluK1-2a: 0.61 ± 0.10, +Neto1: 1.14 ± 0.14 *P=0.0338, +Neto2: 1.37 ± 0.10 **P= 0.0022). However, they did not significantly increase it for GluK1-1a (GluK1-1a: 0.96 ± 0.11, +Neto1: 1.16 ± 0.09 P=0.1880, +Neto2: 0.80 ± 0.05 P=0.2401) and did not show differential modulation (Figure 3E & 3F; Table 1).
We also calculated desensitization and deactivation kinetics in excised outside-out patches. However, GluK1-1a receptors when expressed alone, exhibited low peak amplitudes in outside-out recordings that prevented reliable calculation of gating kinetics. Hence, we only compared properties of receptors co-expressed with Neto proteins and the results obtained were consistent with those obtained from whole-cell recordings. Neto 2 slowed down desensitization of GluK1-1a by ∼ 1.5 times compared to GluK1-2a (ƮDes, GluK1-1a +Neto2: 31.89 ± 4.08 ms; GluK1-2a +Neto2: 20.91 ± 2.11; P=0.0665) (Figure 3G, Table 2). The desensitization rates for GluK1-1a and GluK1-2a receptors coexpressed with Neto1 was also significantly altered (ƮDes, GluK1-1a +Neto1: 4.83 ± 0.46 ms; GluK1-2a +Neto2: 2.84 ± 0.35; *P=0.0310) (Figure G, Table 2. Faster solution exchange times in excised patch recordings allowed us to also measure deactivation kinetics using 1 ms application of 10 mM glutamate. Surprisingly, unlike desensitization, for receptors coexpressed with Neto2, the deactivation rate of GluK1-1a is significantly faster compared to that of GluK1-2a (ƮDea, GluK1-1a +Neto2: 5.18 ± 0.65 ms; GluK1-2a +Neto2: 10.74 ± 1.48; **P=0.0077). In contrast, Neto1 did not significantly alter deactivation kinetics of both GluK1 variant receptors (ƮDea, GluK1-1a +Neto2: 2.83 ± 0.20 ms; GluK1-2a +Neto2: 2.14 ± 0.37; P) (Figure 3H, Table 2). Thus, both whole-cell and excised patch recordings confirm the unique functional properties and differential modulation by Neto proteins due to the presence of fifteen amino acid insert in GluK1-1a receptors.
Mutations in GluK1-1a splice insert alter channel properties
Since our electrophysiological analysis revealed functional differences between the two splice variants and their modulation by Neto proteins, we generated receptors with splice residue mutants and performed functional assays to identify key residues. The splice insert (KASGEVSKHLYKVWK) is dominated by positively charged residues and contains four lysins and one histidine. We hypothesized that these charged residues might affect the interactions at the ATD-LBD interface and influence receptor functions. To investigate this, we prepared charge-reversal (K/H to E) and charge neutral mutants (K/H to A) (Figure 4-table supplement 1) and carried out functional assays. Our cell surface biotinylation assay showed that all mutants (glutamate or alanine) reached the cell surface efficiently (data not shown). However, the charge neutral mutants (K/H to A) gave either very low peak amplitudes (<40 pA) or were not functional, and hence, were not included in the study. The charge reversal mutants K368-E, and K375/379/382H376-E revealed fascinating insights into the role of splice residues in altering GluK1 receptor properties (Figure 4A). Interestingly, both mutants, K368-E and K375/379/382H376-E exhibited a significantly slower rate of glutamate-evoked desensitization compared to wild-type GluK1-1a (ƮDes, GluK1-1a: 5.21 ± 0.50 ms; K368-E: 7.89 ± 1.14 ms *P=0.0334; K375/379/382H376-E: 9.61 ± 1.47 *P=0.0290) (Figure 4B; Table 1. We also observed a significant delay in the recovery from desensitized state for K368-E mutant (K368: 5.61 ± 0.95 s *P=0.0417) compared to wild-type GluK1-1a. In addition, K375/379/382H376-E mutant also exhibited a slowdown in the recovery (K375/379/382H376-E: 4.83 ± 0.31 s P=0.2774) (Figure 4C; Table 1). Our investigations of glutamate-and kainate-evoked responses for wild-type and mutant receptors considering their peak amplitudes (IK/IG) revealed a significant decrease for the K368-E mutant (GluK1-1a: 1.51 ± 0.13; K368-E: 0.81 ± 0.13 **P=0.0037) and a reduction was observed for K375/379/382H376-E receptors (1.17 ± 0.28 P=0.3733) compared to wild-type (Figure 4D; Table 1). This observation is reciprocal to the effect of splice when compared to the non-spliced form indicating importance of these residues in influencing receptor desensitization and recovery. A similar reversal in trend was also observed for the measurements of rectification index for these mutants at positive and negative potentials (+90 mV and -90 mV). The rectification index was significantly reduced in the case of mutant K375/379/382H376-E (K375/379/382H376-E: 0.62 ± 0.14 *P=0.0499). Surprisingly, no outward rectification was observed for the K368-E mutant and must be further investigated to fully understand the reasons (Figure 4E; Figure 5-figure supplement 2C; Table 1).
GluK1-1a splice residues K368, K375, H376, K379 and K382 influence receptor modulation by Neto proteins
Next, we investigated the effects of splice mutants on receptor modulation by Neto proteins. To test whether mutations in splice residues disrupted interactions with Neto proteins, we performed receptor pull-downs using an antibody against the His-tag of the receptor. Our results showed that the mutant receptors could efficiently pull down Neto1 (detected using the Neto1 antibody) and Neto2 (detected using the GFP antibody) (Figure 5-figure supplement 1) suggesting that mutants don’t completely abolish GluK1-1a and Neto interactions.
Furthermore, we conducted experiments using electrophysiology to investigate whether coexpression of Neto proteins can restore the functionality and influence the functions of splice mutants. We observed that mutants K368-E and K368/375/379/382H376-E, desensitize significantly slower in the presence of Neto1 (ƮDes, GluK1-1a +Neto1: 3.56 ± 0.22 ms; K368-E +Neto1: 4.37 ± 0.25 ms *P=0.0393; K375/379/382H376-E +Neto1: 3.74 ± 0.20 ms P=0.5390; K368/375/379/382H376-E +Neto1: 4.86 ± 0.67 ms P=0.1242) (Figure 5A; Figure 5-figure supplement 2A; Table 1). This observation suggests that GluK1-1a modulation by Neto1 is influenced by the splice residues. On the other hand, Neto2 does not have a significant effect on the desensitization of these mutant receptors compared to wild-type-Neto2 (Figure 5A; Figure 5-figure supplement 2A; Table 1).
Similarly, K368-E and K368/375/379/382H376-E mutants recover significantly faster from the desensitized state when coexpressed with Neto1. On the other hand, the recovery from the desensitized state is slower on coexpression of mutants with Neto2. Thus, the pattern of mutant receptor recovery from desensitized state is comparable to that of wild-type receptors, indicating that K368-E and K375/379/382H376-E mutants do not influence receptor recovery (Figure 5B; Table 1).
Furthermore, to determine whether the agonist efficacy of mutant receptors changed in the presence of Neto proteins, IK/IG ratios were measured. Neto1 increased the agonist efficacy for the K368-E and K375/379/382H376-E mutants (K368-E +Neto1: 6.99 ± 0.47 ***P=0.0002; K375/379/382H376-E +Neto1: 1.69 ± 0.15 *P=0.0326; K368/375/379/382H376-E +Neto1: 1.15 ± 0.20 P=0.6495) (Figure 5C; Figure 5-figure supplement 2B; Table 1). Similarly, Neto2 also considerably increased the IK/IG values for mutant K368-E, rescuing the kainate efficacy (K368-E +Neto2: 2.13 ± 0.13 ***P=0.0007), while it does not seem to have any significant effect on the K375/379/382H376-E mutant (K375/379/382H376-E +Neto2: 0.86 ± 0.08 P=0.2045) (Figure 5C; Figure 5-figure supplement 2B; Table 1).
Consistent with the observation above, our examination of the rectification index revealed a significant increase in outward current for K368-E mutant (K368-E +Neto1: 2.84 ± 0.16 **P=0.0021). However, K375/379/382H376-E did not show any difference compared to wild-type receptors, while K368/375/379/382H376-E displayed a decrease in the outward current (K375/379/382H376-E +Neto1: 1.23 ± 0.07 P=0.5351; K368/375/379/382H376-E +Neto1: 0.59 ± 0.13 **P=0.0081) (Figure 5D; Figure 5-figure supplement 2C; Table 1). Interestingly, similar to Neto1, Neto2 was also able to rescue the outward rectification of the K368-E mutant (K368-E +Neto2: 0.76 ± 0.26), suggesting the importance of this residue in receptor modulation by Neto proteins (Figure 5D; Figure 5-figure supplement 2C; Table 1).
Thus, our analysis of the gating properties of GluK1-1a mutants co-expressed with Neto proteins suggests that positively charged residues at positions 368, 375, 376, 379, and 382 in the splice insert influence receptor modulation by Neto proteins. While Neto1 could primarily influence receptors with K/H to E splice mutations, Neto 2 did not show such differential effects and could not influence the gating properties of the mutants studied here significantly. This suggests that while the modulation of the receptor by Neto 1 is affected by mutations in splice insert, the modulation by Neto 2 remains largely unaffected.
The structure of GluK1-1aEM shows an overall conserved architecture of desensitized state in kainate receptors
To evaluate the effects of splice residues on domain organization and structure of GluK1-1a receptors we pursued its structure determination via single particle cryo-EM. Construct optimization was carried out to improve the expression and stability of purified protein. Briefly, the free cysteines in the TM1 region were mutated (C552Y, C557V) based on the sequence analysis with kainate and AMPA receptors, and this construct was named as GluK1-1aEM (Figure 6-figure supplement 1 and 2). The whole-cell patch clamp showed that GluK1-1aEM was functional (Figure 6-figure supplement 3).
The structures of GluK1-1aEM were determined using single-particle cryo-EM. The receptors were either DDM solubilized or reconstituted in lipid nanodiscs and trapped in a desensitized state using 2 mM of high-affinity agonist 2S, 4R-4-methyl glutamate (SYM2081) (Figure 6-figure supplement 4). A resolution of ∼5.2 Å was achieved for the receptors in lipid nanodiscs, but the transmembrane region was not resolved due to an orientation bias (Figure 6; Figure 6-figure supplement 5; Figure 6-table supplement 1). The full-length receptor in detergent micelles had a resolution of 8.2 Å, including the transmembrane region, which was ∼8 Å for the extracellular domain (Figure 6-figure supplement 5; Figure 6-table supplement 1).
A tetrameric receptor model was built based on the crystal structures of GluK1-1a ATD, GluK1 LBD (kainate-bound state; PDB:3C32), and the TM domain based on a highly identical GluK2EM (PDB:5KUF). Our cryo-EM map represented ATD residues-1-398, but the density corresponding to the ATD splice (368-382) was poorly resolved. The ATD-LBD linkers were resolved for all subunits (A to D) in both structures, the S1 and S2 domains were built entirely and the TMD (TM1, TM3 and TM4) was built only for detergent-solubilized receptors (Figure 6; Figure 6-figure supplement 6 and 7). For receptors reconstituted in lipid nanodiscs, we observed only the TM3 bundle. TM2 was not resolved in either dataset (Figure 6; Figure 6-figure supplement 7). Extra densities were observed in the ECD layer of the GluK1-1aEM ND map, which coincided with potential N-linked glycosylation sites (Figure 6-figure supplement 8). GluK1-1aEM maps showed general conservation of the architecture of kainate receptors captured in the desensitized state (Khanra et al., 2021; Kumari et al., 2019; Meyerson et al., 2016; Selvakumar et al., 2021). Consistent with earlier studies on homomeric and heteromeric KARs in the desensitized state, GluK1-1a exhibited a modular organization with three layers, namely, the two-fold symmetric ATD, quasi-four-fold symmetric (LBD and four-fold symmetric TMD. The presence of the ATD splice insert in GluK1-1a did not affect the arrangement of the receptor domains in the desensitized state (Figure 6; Figure 6-figure supplement 7).
Alternative splicing is a well-known mode of protein function modulation in various ion channels, such as transient receptor potential (TRP) (Gracheva et al., 2011; Zhou et al., 2013), big potassium (BK) (Chen et al., 2005), acid-sensing sodium (ASICs) (Bässler et al., 2001), and Shaker K+ channels (Hoshi et al., 1991). In the case of iGluRs, the 38 amino acid residue preceding TM4, known as flip and flop isoforms, is a well-characterized module of AMPARs that affects receptor expression, and gating kinetics and is involved in various pathophysiology (Park et al., 2016; Sommer et al., 1990; Stine et al., 2001). For kainate receptors, the combination of different subunits (GluK1-GluK5) and post-transcriptional modifications, such as RNA editing and splicing provides a broader range of pharmacological and gating properties, which can affect synaptic physiology (Kumar et al., 2011; Kumar and Mayer, 2010; Lerma, 2006; Straub et al., 2016). GluK1 is the most diversified subunit of KARs due to multiple post-transcriptional events and has been widely studied as a potential drug target. A recent report highlighted the equivalent presence of GRIK1-1 (exon 9) with respect to GRIK1-2 (lacking exon 9) (Herbrechter et al., 2021). The dominant presence of the GRIK1-1 gene was also reported in retinal Off bipolar cells of ground squirrel. Interestingly, a N-terminal splice (exon 5) in a similar position has been observed in the GluN1 subunit of NMDA receptors which is known to influence the interactions at the ATD-LBD interface, and therefore proton sensitivity and channel kinetics (Regan et al., 2018). However, this is the first report to decipher the role of the N-terminal splice insert in the kainate receptor family.
Our study compared the role of ATD splice in the kinetics of the GluK1-1a to a previously extensively characterized equivalent receptor without the splice region, GluK1-2a (Copits et al., 2011; Fisher, 2015; Fisher and Fisher, 2014; Sommer et al., 1992; Swanson and Heinemann, 1998). We found that the presence of splice insert affects the desensitization, recovery from desensitization, glutamate sensitivity, and channel rectification of the GluK1 receptor. Moreover, the splice also had a profound impact on desensitization with kainate, suggesting that the receptor follows different functional pathways for the two agonists. Our results showed a significant deviation from GluK1-2a in kainate-versus glutamate-evoked currents (IK/IG), implying a role for splice residues in imparting higher efficacy for kainate. This likely explains the enhanced stability of the kainate-bound state in GluK1-1a, leading to slower desensitization compared to GluK1-2a. Our functional assays of GluK1-1a receptors co-expressed with Neto proteins showed that Neto1 facilitates faster recovery from the desensitized state, consistent with previous reports (Copits et al., 2011; Fisher, 2015; Palacios-Filardo et al., 2016). However, we did not observe the fast onset of desensitization previously reported for GluK-2a (Copits et al., 2011; Fisher, 2015).
Additionally, our results show that Neto2 retards recovery from desensitization for both GluK1 variants, contradicting earlier reports of conflicting recovery rates with Neto2 for GluK1-2a. This indicates that Neto1 and Neto2 may interact with both GluK1 variants in a mutually exclusive manner, or that the splice position may regulate the modulation behavior of Neto2 and Neto1. Our comparison of kainate and glutamate efficacies for the two variants also showed differential modulation by Neto proteins. Both Neto1 and Neto2 reduced the IK/IG ratios in GluK1-1a, while they significantly increased the IK/IG ratios in GluK1-2a, highlighting the impact of the splice insert on receptor response to the agonists (Figure 3D; Figure 3-figure supplement 1B; Table 1).
Our mutational analysis showed that K368, a splice insert residue, affects channel kinetics. The charge reversal mutant (K368-E) showed significant differences from the wild-type GluK1-1a for all tested properties, indicating a role for K368 in protein-protein and/or protein-glycan interactions at the ATD-LBD interface.
Although our cryo-EM map poorly resolved the splice region, its position can be ascertained close to the ATD-LBD interface. Based on our functional assays, the splice seems to affect the interaction between the receptor and auxiliary proteins. The modulatory effects of Neto1 and Neto2 on GluK1 splice variants might be mediated by multiple conserved positively charged patches (Li et al., 2019; Vinnakota et al., 2021). The complex between GluK2-Neto2 (He et al., 2021b) provides a model that suggests K183 and K187 of GluK1 can potentially interact with a negative patch on Neto1 (D140-E144) and Neto2 (D144-E148). However, the splice insert appears to be positioned away from this interacting surface. Thus, it is plausible that the splice residues could come in contact with Neto proteins during a different conformation of the receptor during gating. Additionally, splice residues could also have an indirect or allosteric influence on the modulation of receptor functions and regulation by Neto proteins.
Our research, which encompasses structural, biochemical, biophysical, and functional investigations, highlights the significance of the unique N-terminal splice insert in the functions of GluK1 kainate receptors and opens avenues for further studies to understand its physiological effects. We also elucidated the important residues within the splice insert that could impact the modulatory behavior of auxiliary proteins. Our study emphasizes the need to investigate all possible combinations of KAR splice variants to appreciate their contributions at different developmental stages better. This comprehensive understanding of the distribution and functional diversity is essential for a rational therapeutic approach involving kainate receptors.
Materials and methods
Whole-cell patch-clamp electrophysiology
To understand the functional differences between GluK1-1a and GluK1-2a, as well as their modulation by Neto proteins, a whole-cell patch-clamp analysis was performed. HEK293 WT mammalian cells were seeded on siliconized glass coverslips in 35 mm dishes using Dulbecco’s Modification of Eagle’s Medium (DMEM) containing 10 % fetal bovine serum (FBS), 2 mM glutamine, and 10 units/mL Penicillin-Streptomycin. Cells were transfected with GRIK1-1a or GRIK1-2a cloned in pRK7 (in the presence or absence of rNeto1/rNeto2 cloned in IE-pRK8 as indicated) with EGFP expressing plasmid using Xfect (Clontech) according to manufacturer’s instructions. Similar protocols were followed to test the functionality of the GRIK1-1aEM and GRIK1-1a splice mutant constructs. The whole-cell patch-clamp recording was performed with an EPC 10 USB amplifier (HEKA) 24-48 h post-transfection. Cells were lifted using 1.5 mm diameter thin wall glass capillary tubes (30-0066 Harvard Apparatus), pulled to a fine tip with a Sutter P-1000 micropipette puller (Sutter Instruments, Novato, CA) containing internal solution (10 mM HEPES pH 7.4, 100 mM CsF, 30 mM CsCl, 4 mM NaCl, 0.5 mM CaCl2, 5 mM EGTA and 300 mOsm). Cells were continuously perfused with external/bath solution (10 mM HEPES pH 7.4, 150 mM NaCl, 2.8 mM KCl, 1.8 mM CaCl2, 1 mM MgCl2 and 300 mOsm) through a peristaltic perfusion system (Multichannel systems). Current was measured by holding the membrane at -60 mV, using a 2-kHz low-pass filter. Ligands (10 mM glutamate, 1 mM kainate, 2 mM SYM2081, or 10 µM UBP301) were applied through a double-barrelled theta pipette connected with an ultra-fast piezo-based perfusion system (Multichannel systems) via v8 Perfusion Fast-Step System (VC-77SP). Recordings were controlled and measured using Patchmaster-v2x90.2 (Heka Elektronik). The raw files were analyzed using Clampfit 11.2 and
Fitmaster-v2x90.4. All traces were normalized before being used for calculations. The exponential fit was used to estimate the rate of desensitization (ƮDes) for 100 ms glutamate application, measured as the decline of the current from 80% of its peak amplitude. Mean-weighted Tau (τDes) values were determined using the single exponential, two-term fitting (Levenberg-Marquardt). To compute the recovery from desensitization, a paired-pulse experiment was performed, where the amplitudes of the test pulse were normalized to that of the desensitizing pulse (calculated as relative amplitude); and plotted in comparison to the time between the desensitizing pulse and test pulse in seconds. The rate of recovery (ƮRecovery) was obtained by fitting the one-phase association exponential function. Dose-response experiments were performed for GluK1-1a (co-expressed with or without Neto proteins) and GluK1-2a with different concentrations of glutamate or kainate in the range of 1 µM to 3 mM or 0.5 µM to 600 µM, respectively. Dose-response values were calculated as the percentage of maximum response against log[agonist] concentrations and fitted using variable slope (Hill’s equation) in GraphPad Prism 8.0.1. For calculating kainate efficacy (IK/IG), the ratio of peak amplitudes evoked by kainate versus glutamate was employed. For the calculation of the rectification index, a ratio of peak amplitudes obtained at +90/-90 mV was utilized. Current-voltage (IV) plots were prepared using the voltage ramp from -90 to + 90 mV with a 10 mV increment step, and the current amplitude was normalized to that obtained at -90 mV. For kainate-evoked currents, the percentage desensitization was calculated. The steady-state current measured at the end of 1 s kainate application was divided by peak current. This ratio was then subtracted from 1 and multiplied by 100 to give percentage (%) desensitization (Fisher and Fisher, 2014).
Outside-out patch electrophysiology
HEK 293-T/17 cells were used for outside-out patch experiments 48-96 h post transfection. Cells were transfected with GRIK1-1a or GRIK1-2a cloned in pRK7 (in the presence or absence of rNeto1/rNeto2 cloned in IE-pRK8 as indicated) with EGFP expressing plasmid at DNA ratios of 3:0.5 for receptor alone and 2:8:0.5 with Netos respectively using TransIT®-LT1 Transfection Reagent according to manufacturer’s instructions.
The extracellular solution used for the experiment contained 10 mM HEPES pH 7.3, 150 mM NaCl, 2.8 mM KCl, 2 mM CaCl2, 1 mM MgCl2 and 10 mM glucose, The intracellular solution contained 10 mM HEPES pH 7.3, 110 mM CsF, 30 mM CsCl, 5 mM EGTA, 4 mM NaCl, and 0.5 mM CaCl2.
Patch micropipettes were pulled using a P-97 Sutter puller, and the resistance was maintained at 2.3-2.6 megaohms. After forming the whole-cell configuration, the patch was pulled away from the cell to facilitate an outside-out patch. The cells were voltage-clamped at -70 mV, and a saturated concentration of glutamate (10 mM) was rapidly applied using a three-barrelled theta glass attached to a Siskiyou MXPZT-300 solution switcher. Glutamate applications of 1 ms were used to determine deactivation, while applications of 100 or 1000 ms were used to determine desensitization.
Comparisons between wild-type receptors, EM, or mutant constructs were obtained using an unpaired t-test (two-tailed, with or without the Welch test) or by Brown-Forsythe and Welch ANOVA followed by Dunnett’s multiple comparisons. Statistical analysis was carried out in GraphPad Prism, version 8.0.1. P values < 0.05 were considered statistically significant and are reported (* = p < 0.05, ** = p < 0.01, *** = p < 0.001, **** = p < 0.0001).
Site-Directed Mutagenesis (SDM)
Based on our electrophysiology analysis of the wild-type GluK1-1a/GluK1-2a receptors, structural analysis of GluK1-1aEM, and recent reports that suggest that the presence of the positive patches in GluK2 ATD affects the interaction with Neto proteins (He et al., 2021b; Li et al., 2019; Vinnakota et al., 2021), we performed SDM to understand the role of splice residues in the receptor kinetics. All splice mutations were introduced in the wild-type GRIK1-1a pRK7 construct for electrophysiology, as well as the GRIK1-1aEM-EGFP-His8-pEGBacMam construct for surface expression and pull-downs using the ligation-free cloning approach (Zhang et al., 2017). Clones were confirmed by sequencing. Initially, the positively charged and other residues of the splice were substituted with alanine. Later, charge reversal mutants (K and/or H to E) were also prepared to understand their role in the receptor kinetics as well as interaction with Neto proteins. The mutants prepared are summarized in Figure 4-table supplement 1.
Co-immunoprecipitation (in vitro)
To understand the effect of mutations on GluK1-1a and Neto1/2 interaction, co-immunoprecipitation was carried out using an anti-His monoclonal antibody against the receptor. Similar constructs and transfection protocols were followed for surface expression analysis. Cells were pelleted 65-70 h post-transfection and washed with TBS (20 mM Tris pH 8, 150 mM NaCl). These cells were sonicated and solubilized in 500 uL lysis buffer (20 mM Tris pH 8, 150 mM NaCl, 1% glycerol, protease inhibitor cocktail, 30 mM DDM). Post solubilization, debris was removed by centrifuging at 17,000 x g for 45 minutes at 4 °C. The supernatant was incubated for pre-clearing with 20 µL of pre-equilibrated Protein A agarose beads (Thermo Scientific) for 1 h on a rotator at 4 °C. Post-pre-clearing, ∼ 10% sample was saved as input, and the rest was used for pull-downs. Simultaneously, an antibody (anti-His, Cell Signaling Technology) was added to 40 µL pre-equilibrated Protein A agarose (Thermo Scientific) and incubated for 1 h at 4 °C, followed by the addition of pre-cleared lysate. It was further incubated at 4 °C overnight (14-16 h). The unbound fraction was removed and washed four times with 500 µL wash buffer (20 mM Tris pH 8, 150 mM NaCl, 1% glycerol, 0.75 mM DDM) to remove non-specific interactions. Protein was eluted in 30 µL elution buffer (100 mM Tris pH 6.8, 12% glycerol, 4% SDS, 10 mM DTT, 2% β-mercaptoethanol) by heating at 95 ° C for 10 minutes. Rabbit IgG controls were set up to confirm the validity of the experiment. To analyze the pull-down, 8% SDS-PAGE followed by western transfer was performed. The immunoblots were probed using anti-actin (Sigma), anti-His (Cell Signaling Technology), and anti-Neto1 (Sigma)/anti-GFP (Sigma) to detect the internal control (actin), the receptors and the co-immunoprecipitated Neto proteins respectively.
Construct design for Expression and purification of GluK1-1aEM
To obtain functional GluK1 receptors, rat GRIK1 with ATD splice insert and the shortest C-terminal domain, GRIK1-1a (1-871 amino acid residues), was cloned in the pEGBacMam vector. The receptor was cloned in-frame with a thrombin recognition site (LVPRGSAAAA), EGFP (A207K; non-dimerizing mutant), and His8 at the C-terminus. The wild-type protein generated very low amounts of the tetramer, as observed in fluorescence-assisted size-exclusion chromatography (FSEC). Therefore, based on the alignments of the sequence with GluK2EM, GluK3EM and GluA2, we mutated free cysteines in the TM1 region to residues corresponding to those of GluK2EM or GluA2 [1x Cys (C576S), 2x Cys (C552Y, C557V) and 3x Cys (C552Y, C557V, C576S)] to obtain good yields of the tetrameric receptor. All clones were confirmed by restriction digestion and sequencing. The expression of all the mutants was confirmed by immunoblotting against His-tag and FSEC. GluK1-1a with 2x Cys mutations (C552Y, C557V) gave us the best receptor quality as observed in FSEC and therefore was used as GluK1-1aEM for large-scale purification for structural studies.
GluK1-1aEM expression and purification
Three liters of Human embryonic kidney (HEK) 293 GnTI- suspension-adapted cultures (∼1.5-2.0 x 106 cells/mL) at 0.5 µg/mL were transfected (or infected with P2 virus) with GRIK1-1aEM plasmid [or virus, prepared in DH10Bac as per established protocol (Goehring et al., 2014)] using polyethyleneimine (PEI-MAX, Polysciences; 1 DNA: 3 PEI w/w) as the transfection agent (or, infected at a multiplicity of infection of ∼2). To boost the protein production, 10 mM sodium butyrate (Sigma) was added 16 h post-transfection/infection, and cultures were incubated at 30°C for protein expression. Cells were harvested 65-70 h after transfection / infection, washed with buffer containing 20 mM Tris pH 8 and 150 mM NaCl, and stored at -80 ° C until further processing. The cell pellet was resuspended (20 mL/L culture volume) in lysis buffer (20 mM Tris pH 8, 150 mM NaCl, and protease inhibitor cocktail, Roche). These resuspended cells were disrupted using sonication (QSonica sonicator, 3 cycles of 90 s; 10 s ON/ 20 s OFF; temperature cut-off: 15 °C). The lysate was clarified using low-speed spin (4307 x g for 20 minutes at 4 °C). The membranes were pelleted using ultracentrifugation (118991 x g for 1 h at 4 °C). Solubilization of membrane fraction was done in buffer containing 20 mM Tris pH 8, 150 mM NaCl, 30 mM DDM (Anatrace, D310LA), 5% glycerol, 10 mM imidazole, and protease inhibitor cocktail for 1 h on rotator at 4 °C. The non-solubilized fraction was separated by centrifugation at 47850 x g for 1 h at 4 °C and 4 mL of cobalt-charged TALON resin (Clontech, Takara) was added to the solubilized fraction for batch binding (3 h at 4 °C). Beads were harvested. The column was packed and washed with wash buffer (20 mM Tris pH 8, 150 mM NaCl, 1 mM DDM, 1% glycerol, 40 mM imidazole) until OD280 reached zero. The bound receptor was eluted with elution buffer (20 mM Tris pH 8, 150 mM NaCl, 1 mM DDM, 1% glycerol, 250 mM imidazole). The peak fractions were pooled, concentrated at 1.3 mg / mL, and digested overnight at 4 ° C with thrombin (1:100 w/w). Simultaneously, purified GluK1-1aEM was also reconstituted in MSP1E3D1 nanodiscs with soybean polar lipids (Avanti Polar Lipids, 541602P) in a 1:2:140 ratio (GluK1-1a: MSP: lipids) following already established protocols (Chen et al., 2017; Gao et al., 2016; Ritchie et al., 2009). The thrombin-digested GluK1-1aEM receptors in DDM, or nanodisc-reconstituted receptors, were further purified via gel filtration (Superose 6 10/300, GE) in buffer containing 20 mM Tris pH 8, 150 mM NaCl, 0.5% glycerol, and 0.75 mM DDM (no detergent for nanodisc protein). The peak fractions were pooled and concentrated to ∼0.6 mg/mL (final DDM concentration, ∼7.5 mM) or ∼0.9 mg/mL GluK1-1aEM in nanodisc. All the affinity elution fractions and final purified protein were confirmed for purity and homogeneity using SDS-PAGE and FSEC, respectively. In the subsequent sections, purified GluK1-1aEM in detergent and nanodisc will be called GluK1-1aEM DDM and GluK1-1aEM ND, respectively.
Cryo-EM sample preparation and data collection
The purified protein was incubated with 2 mM 2S, 4R-4-methyl glutamate (SYM2081) before grid preparation to capture the receptor in the desensitized state. The concentration of SYM2081 was confirmed by electrophysiology, and the stability of the receptor-SYM2081 complex was tested using FSEC.
GluK1-1aEM DDM: Double application of 3 µL protein (∼0.6 mg/mL) SYM2081 complex was carried out on glow-discharged gold grids (R 0.6/1, 300 mesh, Quantifoil). The grids were blotted for 4.5 s and 3.5 s, respectively (0 blot force). Vitrobot temperature was maintained at 12°C with 100% humidity, and the sample was vitrified in liquid ethane. The clipped grids were loaded into a 300 keV Titan Krios microscope equipped with a Falcon III direct detector camera (4k x 4k). Movies were recorded in counting mode with a nominal magnification of 59,000X (pixel size: 1.38 Å), and the defocus range of −2.0 to −3.2 µm increased in steps of 0.3. Each movie comprised 25 frames with a total exposure of 60 s. A dose rate of 0.78 e-/frame was applied, with the total dose being 19.5 e-/Å2.
GluK1-1aEM ND: Double application of 2 µL protein (∼0.9 mg/mL) SYM2081 complex was carried out on glow-discharged gold grids (1.2/1.3, 200 mesh, Quantifoil). Grids were blotted for 3 s and 10 s, respectively, followed by vitrification. The clipped grids were loaded into a 300 keV Titan Krios microscope equipped with a K2 direct-detector camera (Gatan). The movies were recorded in super-resolution mode with an energy filter (20eV slit) and a pixel size of 1.41 Å. Each movie was composed of 30 frames with a total exposure of 12 s. A dose rate of 1.36 e-/frame was applied, with a total dose of 40.8 e-/Å2.
All movies (GluK1-1aEM DDM-SYM: 1100, GluK1-1aEM ND-SYM: 1535) were motion corrected using UCSF Motioncor2 (Zheng et al., 2017). Bad micrographs were removed manually post contrast transfer function (CTF) estimation using CTFFIND4 (Rohou and Grigorieff, 2015). Manually picked particles (∼1000) were 2D classified and used as templates for autopicking in RELION or cryoSPARCv 3. For GluK1-1aEM DDM-SYM and GluK1-1aEM ND-SYM, the autopicked particles in cryoSPARCv3 were cleaned up with multiple rounds of 2D classification. Particles in the best classes were used for training TOPAZ for automated particle picking. For GluK1-1aEM DDM-SYM, initially, 13,750 particles were picked; post iterative rounds of 2D and 3D classification, 5372 particles were used for final 3D reconstruction. In the case of GluK1-1aEM ND-SYM, initially 1,97,908 particles were picked. Multiple rounds of clean-up using 2D and 3D classification gave 24,531 particles that were used for the final 3D reconstruction.
The final particles were corrected for local motion in cryoSPARCv3, followed by refinement using C1 symmetry for both GluK1-1aEM DDM-SYM and GluK1-1aEM ND-SYM. Since we had less information on TMD in both the detergent and nanodisc forms, as observed in 2D classes, we performed local refinement for ATD and LBD using an ECD mask for GluK1-1aEM DDM-SYM and GluK1-1aEM ND-SYM, which improved map resolution to 8.01 Å and 5.2 Å (0.143 FSC) respectively. For GluK1-1aEM DDM-SYM, local refinement using a mask for full-length structure yielded a resolution of 8.2 Å. The 3D maps were sharpened via cryoSPARCv3 (Punjani et al., 2017) or DeepEMhancer (Sanchez-Garcia et al., 2021) using a mask from the cryoSPARCv3 refinement output. Local Resolution was estimated using BlocRes (Cardone et al., 2013) in cryoSPARCv3 or Phenix1.19.2 (Afonine et al., 2018a).
Tetrameric assembly for the GluK1-1aEM ND-SYM model was built using crystal structures of individual domains (ATD, not yet published, and LBD, PDB: 3C32, GluK1 LBD crystal structure with kainate) fitted into the EM map (5.2 Å) in UCSF Chimera (Pettersen et al., 2004). Further, for building GluK1-1aEM ND transmembrane domain 3 and GluK1-1aEM DDM trans-membrane domain, GluK2 TMD (PDB:5KUF) was used due to high identity (∼95%) for fitting into EM density. Phenix1.19.2 (Afonine et al., 2018b) and Namdinator (Kidmose et al., 2019) were used to improve the model via the rigid body and Molecular Dynamics based flexible fitting, respectively. The final models fit well into the EM map of GluK1-1aEM ND-SYM, GluK1-1aEM DDM-SYM ECD, and FL, respectively, with a definite density for ATD, LBD, and TMD (pre-M1, M1, M3, and M4). Coot 0.9.4 (Emsley and Cowtan, 2004) was used to analyze the final models, and chimera/chimeraX (Pettersen et al., 2021, 2004) was used for figure preparation.
Spatiotemporal distribution of exon 9 of GluK1 using transcriptomics data analysis
To understand the abundance of GRIK1-1 splice in the human brain, we resorted to RNA-Seq data from the BrainSpan atlas that constitutes various databases to study transcriptional mechanisms in human brain development. The RNA-Seq data were downloaded (https://www.brainspan.org/rnaseq/gene/1099967), plotted in Excel, and analyzed using RStudio (https://www.rstudio.com/) to determine the presence of GluK1 in different regions of the brain at different developmental stages. Further, we narrowed it down to the GRIK1-1 splice (exon 9; start position 30968845, 45 nucleotides in length) and tried to understand how it overlaps with the entire GRIK1 gene expression. These data explored the presence of the ATD splice irrespective of which C-terminal splice variant is present.
We thank Dr Mark L. Mayer and Dr. Sagar Chittori, National Institute of Child Health and Human Development, National Institutes of Health, Bethesda, USA for kindly sharing the co-ordinates and maps of GluK1-1a ATD which were used to generate the tetrameric receptor model. We also thank Dr. Mayer for his critical reading of the manuscript and his feedback. Dr. Eric Gouaux kindly provided the pEG BacMam vector. Access to EM was provided by the National Electron cryo-microscopy facility at the Bangalore Life Sciences Cluster. We thankfully acknowledge the kind assistance of Dr. Vinothkumar Kutti Ragunath, NCBS, Bangalore in grid preparation and EM data collection.
Core Research Grant from the Science and Engineering Research Board, Department of Science and Technology, Govt. of India CRG/2020/003971 (JK) National Centre for Cell Science, Pune for a senior research fellowship (SD)
SD optimized GluK1-1a construct, expressed and purified protein, carried out molecular biology, biochemical experiments, and processed EM data, RV and PMC carried out all the electrophysiology experiments. Janesh Kumar supervised the overall project design and execution. SD, PMC, and JK analyzed data and wrote the manuscript. All authors approved the final draft.
Conceptualization: JK; Methodology: SD, PMC, RV, JK; Investigation: SD, PMC, RV, JK; Visualization: SD, PMC, RV, JK; Funding acquisition: JK; Project administration: JK; Supervision: JK; Writing – original draft: SD, PMC, JK; Writing – review & editing: SD, PMC, JK
Authors declare that they have no competing interests.
Data and materials availability
The cryo-EM density reconstructions and final models were deposited in the Electron Microscopy Data Base (accession codes EMD-34076, EMD-34083, and EMD-34197) and the Protein Data Bank (accession codes 7YSJ, 7YSV, and 8GPR). All other relevant data supporting the key findings of this study are available in the article and its Supplementary Information files or from the corresponding author upon request.
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