Membrane Guanylate Cyclase catalytic Subdomain: Structure and Linkage with Calcium Sensors and Bicarbonate

Membrane guanylate cyclase (MGC) is a ubiquitous multi-switching cyclic GMP generating signaling machine linked with countless physiological processes. In mammals it is encoded by seven distinct homologous genes. It is a single transmembrane spanning multi-modular protein; composed of integrated blocks and existing in homo-dimeric form. Its core catalytic domain (CCD) module is a common transduction center where all incoming signals are translated into the production of cyclic GMP, a cellular signal second messenger. Crystal structure of the MGC’s CCD does not exist and its precise identity is ill-defined. Here, we define it at a sub-molecular level for the phototransduction-linked MGC, the rod outer segment guanylate cyclase type 1, ROS-GC1. (1) The CCD is a conserved 145-residue structural unit, represented by the segment V⁸²⁰-P⁹⁶⁴. (2) It exists as a homo-dimer and contains seven conserved catalytic elements (CEs) wedged into seven conserved motifs. (3) It also contains a conserved 21-residue neurocalcin δ-modulated structural domain, V⁸³⁶-L⁸⁵⁷. (4) Site-directed mutagenesis documents that each of the seven CEs governs the cyclase’s catalytic activity. (5) In contrast to the soluble and the bacterium MGC which use Mn²⁺-GTP substrate for catalysis, MGC CCD uses the natural Mg²⁺-GTP substrate. (6) Strikingly, the MGC CCD requires anchoring by the Transmembrane Domain (TMD) to exhibit its major (∼92%) catalytic activity; in isolated form the activity is only marginal. This feature is not linked with any unique sequence of the TMD; there is minimal conservation in TMD. Finally, (7) the seven CEs control each of four phototransduction pathways- -two Ca²⁺-sensor GCAPs-, one Ca²⁺-sensor, S100B-, and one bicarbonate-modulated. The findings disclose that the CCD of ROS-GC1 has built-in regulatory elements that control its signal translational activity. Due to conservation of these regulatory elements, it is proposed that these elements also control the physiological activity of other members of MGC family.

Introduction

At the time of discovery (Paul et al., 1987) and molecular cloning of the first membrane guanylate cyclase (MGC), ANF-RGC’s (Chinkers et al., 1989; Lowe et al., 1989; Duda et al., 1991; reviewed in Sharma, 2002, 2010) hydropathic analysis predicted that the protein is composed of three general domains: Extracellular (ExtD), Transmembrane (TMD), and Intracellular (ICD). ICD was further subdivided into two vaguely defined domains, N-terminal KHD (Kinase Homology Domain) and C-terminal catalytic domain. Progression in the field refined this overly simplistic demarcation of these two ICD sub-domains (reviewed in Sharma and Duda, 2014) and demonstrated that KHD terminology is imprecise because it refers to a broad and complex regulatory structure. Notably, at the time it was named so because it showed significant sequence identity with the family of tyrosine protein kinases. It was later realized that the original KHD region contained at its C-terminus a 43-residue α-helical region that does not bear any sequence identity with the tyrosine kinases, hence it was not part of the KHD but independent, distinct domain of the guanylate cyclase.

It was proposed that this inter-domain region, wedged between the KHD and the catalytic domain, constitutes the dimerization domain (DD) (Garbers, 1992). It is conserved among the MGC family and functionally causes dimerization of the catalytic domain transforming it into catalytically active form (Wilson and Chinkers, 1995). This concept was then broadened and applied to define the mechanism by which it regulates the activity of ROS-GC1 (Ramamurthy et al., 2001). The central theme of this concept was that the native isolated catalytic domain exists in its inactive form and DD transforms it into an active dimeric form.

Later studies demonstrated that this concept is not valid. The isolated form of the recombinant ROS-GC’s catalytic domain, G⁸¹⁷-Y⁹⁶⁵, without so called DD, is intrinsically homodimeric and is biologically active (Venkataraman et al., 2008), similar is the case with the catalytic domain of STa-RGC (Saha et al., 2009). The current consensus is that the initially named DD is a conserved five-heptad linker region which is universally present between two signaling domains, and accordingly, it has been termed signaling helix domain (SHD) (Anantharaman et al., 2006). The conclusion is that SHD does not govern the dimerization state of the MGCs, and the catalytic domain devoid of this domain exists as a dimer in its natural and crystal states (Rauch et al., 2008; Venkataraman et al., 2008; Winger et al., 2008; Saha et al., 2009). Thus, SHD is not a signature DD and has no role in the basal catalytic activity of a guanylate cyclase. Consequently, a correction has been made in our earlier illustration (Figure 4 of Sharma et al., 2016). In the newly presented illustration SHD has been depicted in its monomer form (Figure 1).

FIGURE 1

FIGURE 1. Modular composition of the ROS-GC1 dimer. (A) A 56 amino acid leader sequence (LS) precedes the extracellular domain (ExtD) in the nascent, immature protein. All signaling events occur in Intracellular Domain (ICD), which is separated from ExtD by transmembrane domain (TMD). ICD is composed of the following domains: juxtamembrane (JMD), kinase homology (KHD), signaling helix (SHD), catalytic core (CCD) and C-terminal extension (CTE). (B) ICD view expanded. Two specific switches for Ca²⁺ sensing subunits, one for GCAP1 in the JMD, and one for GCAP2 in the CTE, are located on opposing sides of the CCD. The S100B sensing site partially overlaps with that for GCAP2. Neurocalcin δ (NCδ) and CO₂/bicarbonate recognition sites are within the CCD. The MGC complex exists as a homodimer. (C) Phototransduction-linked pathways. ROS-GC1 is linked with phototransduction through four distinct pathways: two modulated by Ca²⁺-sensors, GCAP1 and GCAP2; one by Ca²⁺-sensor, S100B and, the fourth, by Ca²⁺-independent CO₂/bicarbonate. The migratory patterns of these pathways from their sites of origin to the CCD are indicated by arrows.

Core Catalytic domain (CCD)

Originally, in ANF-RGC, the entire stretch beyond the “KHD” was termed as CCD (Chang et al., 1989; Chinkers and Garbers, 1989; Chinkers et al., 1989; Lowe et al., 1989; Duda et al., 1991). However, discovery of the ROS-GC subfamily changed this picture. There, CCD was followed by an extra C-Terminal Extension (CTE) sequence (Goraczniak et al., 1994) where the targeted sites of its two Ca²⁺ sensors, GCAP2 and S100B, were present (Duda et al., 2002, 2005). Thus, in the structural paradigm shift the CCD of ROS-GC is sandwiched between the N-terminal SHD and C-terminal CTE domains (Figure 1C); in this environment, CCD is able to transduce three types of phototransduction linked [Ca²⁺] signals: one, generated upstream by GCAP1, second and third generated downstream by GCAP2 and S100B (Figure 1; Duda et al., 2016). With an additional clue that within the CCD resides the targeted site of another Ca²⁺ sensor, neurocalcin δ (NCδ) (Kumar et al., 1999; Venkataraman et al., 2008) (Figure 1B), the signal transduction role of CCD expanded. CCD was no longer merely a translational center of all effector signals, it was also the regulatory element, meaning, it is a complex Ca²⁺-signaling translating element.

Guided by these cues, the boundary and the newer functional roles of CCD were reexamined. The recombinant ROS-GC1 fragment, M⁷³³-K¹⁰⁵⁴ was chosen for detailed analysis (Venkataraman et al., 2008). The key findings were that: (i) CCD represents the G⁸¹⁷-Y⁹⁶⁵ segment of the guanylate cyclase; (ii) the segment is homo-dimeric in nature; and (iii) it contains an ⁸⁴⁴MSEPIE⁸⁴⁹ NCδ regulatory motif. Incorporation of these principles in the fold recognition model of the dimeric form of CCD disclosed that CCD consists of eight β strands and six α-helices (Venkataraman et al., 2008). Its prominent feature is that the two CCD chains are antiparallel, a feature later confirmed experimentally (Duda et al., 2012b). In general, it supported its previously proposed homology-based three-dimensional CCD 1AWL model (Liu et al., 1997), yet it incorporated a significant advancement. An additional seven-residue ⁹¹¹TFRMRHM⁹¹⁷ helix motif in CCD structure was present which represented the docking site, ⁸³⁶V-L⁸⁵⁷ (previously mis-numbered as ⁸³⁷V-L⁸⁵⁸) between ROS-GC1 and NCδ (Venkataraman et al., 2008).

As of to-date, no crystal structure of any MGCs CCD module exists. However, subsequent to (Venkataraman et al., 2008) publication, crystal structures of CCD of the two forms of guanylate cyclases have been solved, eukaryotic (Cyg12) unicellular green algae Chlamydomonas reinhardtii (Winger et al., 2008) and Cya2 cyanobacterium Synechocystis (Rauch et al., 2008). Cyg12 represents atypical soluble and Cya2 the bacterium MGC.

With the model system of the recombinant ROS-GC1 the present study decodes the precise structure of its CCD, elucidates its biochemical principles at the sub-molecular level, through experimentation validates them for its regulation by Ca²⁺ sensors GCAP1, GCAP2 and S100B and bicarbonate operative in phototransduction, and finally, proposes their application to the general MGC family.

Materials and Methods

Molecular Modeling

Three-dimensional model of ROS-GC1 CCD monomer was built using structural information on eukaryotic soluble guanylate cyclase (Cyg12) CCD of the green algae Chlamydomonas reinhardtii (Winger et al., 2008) as a template, UniProt entry P55203 with A1013R as the query sequence, and Iterative Threading and ASSEmbly Refinement, I-TASSER (web server version)¹. The top-3 unique templates identified by I-TASSER were (PDB IDs), 3uvj_A, 3et6_A and 4p2f_A. Note that 3uvj_A denotes PDBID_ChainName. Based on the secondary structure predictions and I-TASSER C-score, the top-ranked model for CCD was chosen as a representative structure referred to it as the default model for CCD. Two copies of I-TASSER built CCD monomer models were structurally aligned with the experimental soluble guanylate cyclase dimer structure, PDI ID: 3et6 (Winger et al., 2008) to create a homo-dimer ROS-GC1-CCD model. FATCAT² method was used for the structural alignments and creating the dimer model of CCD. The details of the modeling are provided in the Supplemental Materials.

ROS-GC1 Mutants

(1) Point mutations for the creation of the D⁸³⁴A, E⁸⁷⁴A, D⁸⁷⁸A, R⁹²⁵A, C⁹⁴⁶A, N⁹⁵³A, R⁹⁵⁷A, and E⁸⁷⁴A/C⁹⁴⁶A mutants were introduced to ROS-GC1 cDNA by polymerase chain reaction using appropriate mutagenic primers. The mutations were verified by sequencing. (2) Membraneous abridged forms of ROS-GC1: ΔExtD mutant was constructed by introducing two Hpa1 restriction sites at nucleotide positions 241 and 1446 in ROS-GC1 cDNA. The 1.2 kb Hpa1 fragment was excised, and the remaining part re-ligated; ΔExtD,ΔJMD,ΔKHD mutant was constructed from the ΔExtD mutant by introducing two BglII restriction sites at nucleotide positions 1557 and 2503 and excision of a 1 kb BglII fragment (amino acids 447–761); for the ΔSHD mutant two HpaI sites were introduced at nucleotide positions 2533 and 2663 allowing excision of a fragment amino acid residues 772–808; for the ΔCTE mutant a TGA STOP codon was introduced at position 972. (3) Soluble constructs of ROS-GC1: partKHD/SHD/CCD/CTE (aa 733–1054) fragment was amplified by PCR from the ROS-GC1 cDNA by PCR and cloned in frame into pET30a bacterial expression vector; CCD/CTE (aa 817–1054), CCD (aa fragment 817–965), and CTE (aa fragment 986–1054) fragments were amplified by PCR from ROS-GC1 cDNA and cloned in frame into pET30aLIC vector.

Expression of Membraneous ROS-GC1 Mutants in COS Cells

COS-7 cells were induced to express ROS-GC1 or its membrane-bound mutants using a calcium-phosphate coprecipitation technique (Sambrook et al., 1989). Sixty hours after transfection, the cells were harvested and their membranes prepared (Duda et al., 2016). The mutations did not affect membrane targeting of the proteins and their half-lives as verified by immunostaining. Some of the harvested cells were seeded on coverslips, fixed in 4% paraformaldehyde, stained with ROS-GC1 antibody and the immunoreaction was visualized after incubation with secondary antibody conjugated with DyLight488. The membraneous expression of the mutants was comparable.

Expression of Soluble ROS-GC1 Constructs

The soluble ROS-GC1 constructs were individually expressed in BL21 bacterial cells as a His-tag fusion proteins and purified by Ni affinity chromatography. Purity of the protein was analyzed by SDS-PAGE. Concentration of the protein was determined by Bradford method at A₆₀₀.

Assay of Guanylate Cyclase Activity

Membrane samples were incubated individually without or with varying concentrations of recombinant bovine GCAP1 or GCAP2 (purified as described in Duda et al., 2011), recombinant mouse S100B (purified as in Pozdnyakov et al., 1997) or NaHCO₃. The assay mixture (25 μl) consisted of (mM): 10 theophylline, 15 phosphocreatine, and 50 Tris-HCl; pH 7.5, and 20 μg creatine kinase (Sigma). In experiments with GCAP1 and GCAP2, 1 mM EGTA was added to the reaction mixture; with S100B, 1 μM Ca²⁺ was present, and when the bicarbonate effect was tested, neither EGTA nor Ca²⁺ were added. The reaction was initiated by addition of the substrate solution (4 mM MgCl₂ and 1 mM GTP, final concentrations) and maintained by incubation at 37°C for 10 min. The reaction was terminated by the addition of 225 μl of 50 mM sodium acetate buffer, pH 6.2, followed by heating on a boiling water bath for 3 min. The amount of cyclic GMP formed was determined by radioimmunoassay (Nambi et al., 1982). All assays were done in triplicate and except where stated otherwise, were performed three times.

The catalytic activities of the soluble ROS-GC1 deletion mutants were assayed identically, except that purified protein instead of cell membranes was present in the reaction mixture and the cyclic GMP formed was measured by radioimmunoassay.

The guanylate cyclase activity is presented as average ± SD of three experiments done in triplicate.

To correlate the catalytic changes brought about by the mutations, the activities of the mutants were compared with wild type recombinant ROS-GC1 through Michaelis plots for the ligand used, fitting the data to the Hill equation, v = V_max (S)ⁿ/K_M + Sⁿ. V_max is the activity, S is the concentration of the ligand, K_M is the substrate concentration at which half-maximal velocity is achieved, and n is the Hill coefficient.

Results

Membrane Guanylate Cyclase ROS-GC1 Core Catalytic Domain Structure

ROS-GC1 CCD Is a 145-Residue, V⁸²⁰-P⁹⁶⁴, Structural Unit

Through the years since its discovery, the boundaries of the ROS-GC1 CCD have been progressively narrowed down. The first description states that “residues 759 to 1010, cover a region with high degree of sequence identity with the conserved catalytic regions of other guanylate and adenylate cyclases” (Goraczniak et al., 1994). It was later determined that the region beyond Y⁹⁶⁵ of ROS-GC1 does not contribute to the cyclase catalytic activity (Duda et al., 2002), thus this residue marks the CCD C-terminal boundary. The N-terminus of the CCD was determined through activity analyses of abridged forms of ROS-GC1. It was found to be G⁸¹⁷ (Venkataraman et al., 2008).

To verify the precision of setting the ROS-GC1 CCD boundaries to G⁸¹⁷ and Y⁹⁶⁵ as its N- and C-termini, its sequence was aligned with the corresponding CCDs of Cyg12 (atypical soluble) and Cya2 (transmembrane), the first crystalized guanylate cyclase catalytic domains. The alignment demonstrates that the maximally conserved region stretches from ROS-GC1 amino acid residue V⁸²⁰ to P⁹⁶⁴ (Figure 2). This 145-residue region shows 45% identity with the atypical green algae soluble and 12% with the bacterium MGC CCD. The identities between Cyg12 and Cya2 CCDs are 19%. Thus, on the evolutionary ladder the atypical soluble green algae CCD is closer to the mammalian (ROS-GC) CCD than is the bacterial MGC CCD.

FIGURE 2

FIGURE 2. Sequence alignment of ROS-GC1 145 amino acid residues CCD with the corresponding domains of eukaryotic green algae Chlamydomonas reinhardtii (Cyg12) atypical soluble guanylate cyclase and cyanobacterium Synechocystis (Cya2) membrane guanylate cyclase (MGC). The sequences were aligned using Clustal V method. The conserved amino acid residues are marked in red. The numbering of ROS-G1 residues corresponds to the mature protein; of Cyg12 and Cya2 is according to GenBank accession numbers XP_001700847 and Swiss-Prot entry P72951, respectively. The seven critical for catalytic activity residues are marked as: predicted to be involved in Mg²⁺ binding; predicted to be involved in guanine recognition; predicted to be involved in ribose binding; predicted to be involved in triphosphate binding.

Structure-Focused View of the CCD. Inactive and Active States

Because of the higher sequence identity, crystal structure of Cyg12 CCD was chosen as a template to build ab initio a three-dimensional model of ROS-GC1 CCD. The structure of the CCD monomer was modeled by sequential substitution of the Cyg12 residues with those of ROS-GC1 using the I-TASSER modeling suite.

The constructed model shows that the CCD monomer of ROS-GC1 retains the structural features of the class III nucleotide cyclase fold. It covers a 8-stranded β-sheet enclosed by six α-helices (Figure 3A). The monomer contains seven, predicted to be critical for catalytic activity (Liu et al., 1997), residues. Their positions are indicated in Figure 3B. They are: D⁸³⁴ in β1, D⁸⁷⁸ in β2 - β3 loop, N⁹⁵³ in α4, E⁸⁷⁴ in β2, C⁹⁴⁶ in β5, R⁹²⁵ and R⁹⁵⁷ in β4a. It is noteworthy that in the bacterial Cya2 MGC only five of them are conserved (Rauch et al., 2008) (Figure 2). Two residues, corresponding to ROS-GC1, R⁹²⁵ and C⁹⁴⁶, have been substituted by G and E residues (Figure 2).

FIGURE 3

FIGURE 3. ROS-GC1 CCD 3-dimensional model. (A) Monomer model. The model was built de novo using Cyg12 catalytic domain as a template and I-TASSER server. The model is shown in solid ribbon display style and colored using N (blue)-to-C (red) scheme. The secondary structures, eight β-stranded sheets and six α-helices are labeled. Numbering scheme of the β-strands and α-helices is similar to Winger et al. (2008). (B) Localization of CE residues within the CCD monomer. CCD is shown in ribbon style colored in N (blue)-to-C (red) gradient color. The amino acid residues that constitute the catalytic elements (CEs) are identified in the ball-and-stick representation. The Mg²⁺ ion binding residues (D⁸³⁴, D⁸⁷⁸) are shown in red, the ribose binding residue (N⁹⁵³) is shown in green, the two guanine binding residues (D⁸⁷⁴, C⁹⁴⁶) are shown in purple and the two triphosphate binding residues (R⁹²⁵, R⁹⁵⁷) are shown in blue. The residue locations follow UniProt P55203 canonical sequence. (C) CCD dimer. To create the ROS-GC1 CCD homodimer, two copies of the monomer models were independently aligned to separate chains of the Cyg12 catalytic domain dimer (PDB ID 3et6). Protein monomer chains are shown in solid ribbon mode and colored using N-to-C coloring scheme (N-terminus: blue; C-terminus: red; a gradient color from blue through white to red for the intermediate residues). Locations of the CE residues within the dimer are indicated. The dimer possesses two-fold symmetry with a rotational axis that is perpendicular to the plane of the figure. The symmetry is represented by a filled-oval shape placed at the origin and an arrow passing through the plane. (D) Close-up view of the CCD active site. Model of one active site of ROS-GC1 CCD dimer with CE residues shown in a stick mode is depicted. To identify the potential binding site, the ROS-GC1 CCD model was aligned with the experimental mammalian adenylate cyclase structure (PDB: 1CJU).

To create the ROS-GC1 CCD homodimer, two copies of the monomer models were independently aligned to separate chains of the Cyg12 catalytic domain dimer.

In the dimer form the two CCD monomer chains are locked in an antiparallel orientation and are spatially linked by two-fold symmetry axis that runs through the central dimer gap forming a circlet-like structure (Figure 3C). The antiparallel orientation of the two CCD monomers was experimentally documented previously (Duda et al., 2012b). The β1a, β4b, and β5 segments are part of the dimer interface. The central cavity between the two monomers includes two symmetrical active sites. Each active site is formed by critical for catalytic activity residues from both monomers (Figure 3D). In an inactive state the dimer is in an open conformation. It must close to attach the GTP for catalysis to occur. The two active sites in CCD are predicted to act cooperatively (Winger et al., 2008).

Catalytically Active Residues

Guided by the adenylate cyclase crystal structure template (Sunahara et al., 1997), it was predicted, based on human and bovine forms of ROS-GC1 CCD, that its seven residues are critical for the guanylate cyclase catalytic activity (Liu et al., 1997; Venkataraman et al., 2008). [It is, however, noted that the structure used for the modeling of the MGC (Shyjan et al., 1992) by Liu et al. (1997) is erroneous; its correct structure has been subsequently published (Goraczniak et al., 1994).] All these ROS-GC1 residues are present in the 145-residue region of ROS-GC1 CCD (Figures 2, 3B) and are also fully conserved in the Cyg12 CCD (Winger et al., 2008).

It is predicted that these seven catalytic residues collectively control the basal and the ligand-dependent regulatory activities of the guanylate cyclase. In ROS-GC1 their projected functions are as follows: D⁸³⁴ and D⁸⁷⁸ – Mg²⁺ binding; N⁹⁵³ – ribose- positioning; E⁸⁷⁴ and C⁹⁴⁶ – guanine recognition; and R⁹²⁵ and R⁹⁵⁷ – triphosphate-angling, (Figures 2, 3B). They are termed from here on the CCD-Catalytic Element (CE) residues.

Experimental Validation of the Model-Predicted CEs

Photoreceptor ROS-GC1 is linked with phototransduction through its four limbs by distinct pathways: two modulated by Ca²⁺-sensors, GCAP1 and GCAP2; one by Ca²⁺-sensor, S100B and, the fourth by CO₂ (bicarbonate) via a Ca²⁺-independent mechanism (Figure 1C) (reviewed in Sharma et al., 2016). The first two pathways are specific for rod photoreceptors (Makino et al., 2008, 2012; Koch and Dell’orco, 2013); GCAP1- and S100B-modulated for the cone photoreceptors (Wen et al., 2012; Sharma et al., 2014) and the GCAP1 and CO₂/bicarbonate-modulated pathways for the red cone photoreceptors (Duda et al., 2015). Notably, the migratory patterns of these pathways are very different, yet they all are translated to generate cyclic GMP at a common CCD center. The origin and flow of the GCAP1 signal pathway is exceptional, it originates in an intracellular, JMD site and is then successively processed at the KHD and SHD sites before being transmitted to the CCD for final processing operation (Figure 1C). In contrast, GCAP2 and S100B signals originate on the CTE and then are transmitted to the CCD. A ⁶⁵⁷WTAPELL⁶⁶³ motif is critical for the signaling of both GCAPs, however, it has no role in controlling the basal catalytic activity of the cyclase or in the binding of the GCAPs (Duda et al., 2011). Bicarbonate signal, in a unique mode to itself, originates and gets translated at the CCD (Duda et al., 2015, 2016). The CENTRAL POINT is that all the transmitted signals, once they arrive at the CCD, are translated by the identical transduction steps. The functional (regulatory) specificity of the signals resides only in their migratory pathways.

In order to validate the critical role of the model-predicted CE residues in ROS-GC1 function in photoreceptor outer segments, we analyzed the effect of their mutations on the basal and regulatory catalytic modes of the guanylate cyclase. Each residue was individually mutated to alanine and the resulting mutant was assessed for its basal and ligand (Ca²⁺ sensor GCAPs and S100B or Ca²⁺- independent bicarbonate)-dependent activities. Because the site-directed mutation/expression results are very similar for each CE residue, only their combined essentials are provided.

The Mg²⁺ binding residues: D⁸³⁴, CE motif 1; D⁸⁷⁸, CE motif 3. D⁸³⁴ mutation results in the inhibition of 71.3% and D⁸⁷⁸ of 73.7% of basal ROS-GC1 catalytic activities (Figure 4A). Thus, each residue controls more than 70% of the basal saturation activity of ROS-GC1.

FIGURE 4

FIGURE 4. The effect of alanine mutation of Mg²⁺ coordinating residues D⁸³⁴ (CE1) and D⁸⁷⁸ (CE3) on basal and regulated ROS-GC1 activity. COS cells were individually transfected with ROS-GC1 mutants D⁸³⁴A or D⁸⁷⁸A and their membrane fractions were assessed for guanylate cyclase activity. (A) Basal guanylate cyclase activity; (B) GCAP1-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (C) GCAP2-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (D) S100B-dependent activity in the presence of 1 μM Ca²⁺; and (E) bicarbonate-dependent activity. Membranes of COS cells transfected with wild type ROS-GC1 were analyzed identically. The experiment was done in triplicate and repeated three times with different COS cell membranes preparations. The results shown are mean ± SD of these experiments. The error bars are within the size of the symbols.

Connected with these losses, the two mutations also disable all of the ROS-GC1’s four-limbed modulatory activities. GCAP1: D⁸³⁴ mutation lowers the ROS-GC1 V_max from 440 to 71 pmol cyclic GMP min^-1 (mg protein)^-1 and D⁸⁷⁸ mutation to 81 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 4B). The EC₅₀ values (∼0.8 μM) and Hill coefficients (∼2) for both mutants remain unchanged. GCAP2: D⁸³⁴ mutation lowers ROS-GC1 V_max from 504 to 53 pmol cyclic GMP min^-1 (mg protein)^-1 and D⁸⁷⁸ mutation, to 45 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 4C). The EC₅₀ values (∼4 μM) remain the same, yet Hill coefficient values are lowered, to 1.35. S100B: Recall, In contrast to the GCAP sensors, S100B senses and stimulates ROS-GC1 catalytic activity in a Ca²⁺-dependent manner with a K_1/2 of 0.3 to 0.8 μM (reviewed in Sharma et al., 2016). D⁸³⁴ mutation lowers the ROS-GC1 V_max from 452 to 72 pmol cyclic GMP min^-1 (mg protein)^-1 and D⁸⁷⁸ to 91 pmol cyclic GMP min^-1(mg prot)^-1 (Figure 4D). The S100B EC₅₀ value of 0.8 μM and stimulatory Hill’s coefficient of 2 remain unchanged. CO₂: This phototransduction-linked limb of the ROS-GC1 is a recent discovery (Duda et al., 2016; reviewed in Sharma et al., 2016). It is a bicarbonate-modulated Ca²⁺-independent signal transduction pathway. Our scattered ongoing studies have begun to show that this pathway is signaled by CO₂ through carbonic anhydrase (CAII) enzyme, which converts CO₂ to bicarbonate and, bicarbonate, in turn, serves the second messenger of CO₂; importantly, in support of this hypothesis, electric recording studies demonstrate that the carbonic anhydrase inhibitor hinders the bicarbonate-dependent generated electric impulses in the red cones of the salamander (Makino et al., 2017). Like the three Ca²⁺-modulated pathways, the D⁸³⁴A and D⁸⁷⁸A mutations partially disable the bicarbonate modular operation (Figure 4E). D⁸³⁴A mutation lowers the V_max from 465 to 57 pmol cyclic GMP min^-1(mg prot)^-1 and D⁸⁷⁸A to 60 pmol cyclic GMP min^-1(mg prot)^-1. The EC₅₀ values of ∼30 mM bicarbonate remain similar to the 25 mM for the wild type ROS-GC1. The Hill’s coefficients are 1.93 and 1.64 for the D⁸³⁴A and D⁸⁷⁸A mutants, respectively, slightly lower than the 2.3 for ROS-GC1.

The ribose positioning residue, N⁹⁵³, CE motif 6, controls 55% of basal ROS-GC1’s catalytic activity (Figure 5A) and also disables most of the modulatory activities of its four-limbed pathways (Figures 5B–E). GCAP1: N⁹⁵³ mutation lowers the ROS-GC1 V_max from 440 to 95 pmol cyclic GMP min^-1 (mg protein)^-1. The EC₅₀ values (∼0.8 μM) and Hill coefficients (∼2) for both mutants remain the same as for wild type ROS-GC1 (Figure 5B). GCAP2: N⁹⁵³ mutation lowers the ROS-GC1 V_max from 508 to 92 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 5C). The mutation does not affect the EC₅₀ (∼4 μM) and Hill coefficient of 2. S100B: N⁹⁵³ mutation lowers the ROS-GC1 V_max from 452 to 97 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 5D). The EC₅₀ value of 0.8 μM and stimulatory Hill’s coefficient of 2 remains unchanged. CO₂: The N⁹⁵³ mutation results in lowering the ROS-GC1 V_max from 465 to 94 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 5E) but has no effect on EC₅₀ (∼25 mM bicarbonate) and Hill coefficient (2.2) values.

FIGURE 5

FIGURE 5. The effect of ribose binding residue N⁹⁵³ (CE6) mutation to alanine on basal and regulated ROS-GC1 activity. COS cells were transfected with ROS-GC1 mutant N⁹⁵³A and their membrane fractions were assessed for guanylate cyclase activity. (A) Basal guanylate cyclase activity; (B) GCAP1-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (C) GCAP2-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (D) S100B-dependent activity in the presence of 1 μM Ca²⁺; and (E) bicarbonate-dependent activity. Membranes of COS cells transfected with wild type ROS-GC1 were analyzed identically. The experiment was done in triplicate and repeated three times with two different COS cell membranes preparations. The results shown are mean ± SD of these experiments. The error bars are within the size of the symbols.

The triphosphate angling residues R⁹²⁵, motif CE4, and R⁹⁵⁷, motif CE7. They control, respectively, 66 and 53% of basal ROS-GC1 catalytic activity, and also disable most of the modulatory activities of its four-limbed pathways (Figure 6). GCAP1: R⁹²⁵ mutation lowers the ROS-GC1 V_max from 440 to 50 pmol cyclic GMP min^-1 (mg protein)^-1 and R⁹⁵⁷ mutation to 70 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 6B). The EC₅₀ values (∼0.8 μM) and Hill coefficients (∼2) for both mutants remain unchanged, however. GCAP2: R⁹²⁵ mutation lowers the ROS-GC1 V_max from 508 to 63 pmol cyclic GMP min^-1 (mg protein)^-1 and R⁹⁵⁷ mutation to 57 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 6C). The EC₅₀ values (∼4 μM) remain unchanged and also the Hill coefficient value of 2.0. S100B: R⁹²⁵ mutation lowers the ROS-GC1 V_max from 452 to 70 pmol cyclic GMP min^-1 (mg protein)^-1 and R⁹⁵⁷ to 90 pmol cyclic GMP min^-1 (mg prot)^-1 (Figure 6D). The S100B EC₅₀ value of 0.8 μM and stimulatory Hill’s coefficient of 2 remains unchanged. CO₂: Like the three Ca²⁺-modulated pathways, the R⁹²⁵ and R⁹⁵⁷ mutations disable the bicarbonate operation. R⁹²⁵ mutation lowers the ROS-GC1 V_max from 465 to 63 pmol cyclic GMP min^-1 (mg protein)^-1 and R⁹⁵⁷ to 145 pmol cyclic GMP min^-1 (mg prot)^-1 (Figure 6E). The EC₅₀ for bicarbonate is ∼25 mM for both mutants. The Hill coefficient of 1.1 for the R⁹²⁵A mutant is significantly lower than 2.3 for wild type ROS-GC1 but for the R⁹⁵⁷A mutant, 1.7, is close.

FIGURE 6

FIGURE 6. The effect of triphosphate binding residues R⁹²⁵ (CE4) and R⁹⁵⁷ (CE7) substitution with alanine on basal and regulated ROS-GC1 activity. Membranes of COS cells expressing separately two single mutants R⁹²⁵A or R⁹⁵⁷A were assayed for guanylate cyclase activity. (A) Basal guanylate cyclase activity; (B) GCAP1-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (C) GCAP2-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (D) S100B-dependent activity in the presence of 1 mM Ca²⁺; and (E) bicarbonate-dependent activity. Membranes of COS cells transfected with wild type ROS-GC1 were analyzed identically. The experiment was done in triplicate and repeated two times with different COS cell membranes preparations. The results shown are mean ± SD of these experiments. The error bars are within the size of the symbols.

The guanine recognition residues, E⁸⁷⁴, motif CE2 and C⁹⁴⁶, motif CE5. Individually, residues E⁸⁷⁴ and C⁹⁴⁶ control, respectively, 72 and 65% of the basal catalytic activities (Figure 7A) and both mutations together disable all the basal activity of ROS-GC1 (Figure 7A: mutant E⁸⁷⁴A/C⁹⁴⁶A). GCAP1: E⁸⁷⁴A mutation lowers the ROS-GC1 V_max from 440 to 115 pmol cyclic GMP min^-1 (mg protein)^-1 and the C⁹⁴⁶A mutation to 87 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 7B). The EC₅₀ values of ∼0.8 μM are the same as for the wild type ROS-GC1 and the Hill’s coefficients of 1.75 and 1.71 for the mutants are close to the 2 value for the wild type cyclase. The double mutant is unresponsive to any concentration of GCAP1 tested (Figure 7B). GCAP2: Mutation of E⁸⁷⁴ lowers the ROS-GC1 V_max from 508 to 60 pmol cyclic GMP min^-1 (mg protein)^-1 and mutation of C⁹⁴⁶ to 80 pmol cyclic GMP min^-1 (mg protein)^-1 (Figure 7C). The EC₅₀ values (∼4 μM) remain unchanged; the Hill’s coefficients are above 1, but slightly lower than that for wild type ROS-GC1, being 1.57 for the E⁸⁷⁴A mutant and 1.50 for C⁹⁴⁶A. The double mutant does not respond to GCAP2 (Figure 7C). S100B: E⁸⁷⁴A mutation lowers the ROS-GC1 V_max from 452 to 93 pmol cyclic GMP min^-1 (mg protein)^-1 and C⁹⁴⁶A, to 122 pmol cyclic GMP min^-1 (mg prot)^-1 (Figure 7D). The values of EC₅₀ of ∼0.7 μM S100B and the Hill’s coefficients of 1.7 for both mutants are the same as for the wild type ROS-GC1. There is no measurable activity of the double mutant either with or without S100B (Figure 7D). CO₂: Like the three Ca²⁺-modulated pathways, E⁸⁷⁴A and C⁹⁴⁶A mutations affect bicarbonate operation. Mutation of E⁸⁷⁴ lowers the ROS-GC1 V_max from 465 to 54 pmol cyclic GMP min^-1 (mg protein)^-1 and C⁹⁴⁶ to 61 pmol cyclic GMP min^-1(mg prot)^-1 (Figure 7E). The mutations do not affect significantly the EC₅₀ and Hill coefficient values. They remain comparable to the wild type ROS-GC1 values being EC₅₀ ∼30 mM for both mutants and Hill coefficient 1.91 for E⁸⁷⁴A and 1.53 for C⁹⁴⁶A. Importantly, there is no detectable catalytic activity of the double mutant (Figure 7E).

FIGURE 7

FIGURE 7. The effect of substitution of guanine binding residues E⁸⁷⁴ (CE2) and C⁹⁴⁶ (CE5) with alanine on basal and regulated ROS-GC1 activity. Membranes of COS cells induced to express independently two single mutants E⁸⁷⁴A or C⁹⁴⁶A or one double mutant E⁸⁷⁴A/C⁹⁴⁶A were assayed for guanylate cyclase activity. (A) Basal guanylate cyclase activity; (B) GCAP1-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (C) GCAP2-dependent activity in the presence of 1 mM EGTA (10 nM Ca²⁺); (D) S100B-dependent activity in the presence of 1 mM Ca²⁺; and (E) bicarbonate-dependent activity. Membranes of COS cells transfected with wild type ROS-GC1 were analyzed identically. The experiment was done in triplicate and repeated three times with two COS cell membranes preparations. The results shown are mean ± SD of these experiments. The error bars are within the size of the symbols.

An earlier study (Tucker et al., 1998) concluded that both residues, E⁸⁷⁴ and C⁹⁴⁶ (E⁹²⁵ and C⁹⁹⁷, corresponding human ROS-GC1 residues), individually control the total catalytic activity of the ROS-GC1. In this study the authors used the HEK 293 cell system for the expression of guanylate cyclases; and they did not evaluate the mutant with double mutations (E⁹²⁵/C⁹⁹⁷) and the residues were mutated, respectively, to K and D instead of A. Our results revise this conclusion; only two mutations together, E⁸⁷⁴/C⁹⁴⁶, totally disable the catalytic activity of ROS-GC1.

Alanine mutation of CE residues does not affect cooperativity of CCD active sites. Homodimeric antiparallel structure of the guanylate cyclase catalytic domain results in the existence of two equivalent catalytically active sites (Liu et al., 1997; Venkataraman et al., 2008). It was now sought to determine how mutation of an individual CE would affect the communication between the active sites in the mutant-cyclases. Activity assays were carried out in the presence of constant concentration of Mg²⁺ and varying concentrations of GTP (0–3 mM) and K_M as a measure of a mutant’s affinity for GTP and Hill coefficients indicative of interaction between active sites, were determined. The results are summarized in Table 1. For the wild type ROS-GC1 the K_M value for GTP was 0.45 mM. All ROS-GC1 CE mutants exhibited K_M values around 0.5 mM, ranging from 0.48 for D⁸⁷⁸A to 0.64 for C⁹⁴⁶A. As expected, ROS-GC1 exhibited positive cooperativity, with a Hill coefficient of ∼2 (2.01 ± 0.32), conforming the presence of two, interacting with each other, active sites. All the mutants exhibited also positive cooperativity, with Hill coefficients significantly above 1, varying from 1.68 ± 0.22 for C⁹⁴⁶A to 2.11 ± 0.23 for D⁸⁷⁸A. These results demonstrate that although the CE mutations considerably hinder the catalytic processes of the active sites, leading to drastically lowered V_max values, the sites remain cooperative in their catalytic functions.

TABLE 1

TABLE 1. Effect of ROS-GC1 CE mutations on catalytic site characteristics.

These results provide experimental proof that indeed the D⁸³⁴, E⁸⁷⁴, D⁸⁷⁸, R⁹²⁵, C⁹⁴⁶, N⁹⁵³, and R⁹⁵⁷ residues of the ROS-GC1 CCD are critical for the cyclase’s catalytic activity. Although no one mutation individually leads to complete inactivation, they collectively do so. Therefore, each of these residues represents one of the seven structural units of the CE that control full catalytic activity of ROS-GC1.

Is the same true for all MGCs?

The CCD structure along with seven CE residues is conserved in the mammalian MGC family. To determine whether the CE residues are conserved in the MGC family first, the sequence of ROS-GC1 145-residue CCD was compared with the corresponding sequences of the other six members of the family: ROS-GC2, V^829-P⁹⁷⁵; ONE-GC, V^818-P⁹⁶²; ANF-RGC, Q^836-L⁹⁸⁰; CNP-RGC, Q^830-A⁹⁷⁴; STa-RGC, K^794-P⁹³⁵; GC-G, V^849-P⁹⁹³ (Figure 8). The percentile of their sequence identities with ROS-GC1 were: 93, 85, 68, 70, 75, and 69, respectively.

FIGURE 8

FIGURE 8. Conservation of CCD sequence among mammalian MGCs. The sequences of CCD of bovine ROS-GC1 (GC-E), bovine ROS-GC2 (GC-F), rat ONE-GC (GC-D), rat ANF-RGC (NPR-A), human CNP-RGC (NPR-B), human STa-RGC (hSTAR) and rat GC-G were aligned. The names in brackets are the alternate names according to NCBI PubMed. Positions of the amino acid residues of all these MGCs correspond to mature proteins. The conserved amino acid residues are marked in red. The seven critical for catalytic activity residues are marked as: predicted to be involved in Mg²⁺ binding; predicted to be involved in guanine recognition; predicted to be involved in ribose binding; predicted to be involved in triphosphate binding.

To assess and then to formulate a unified signal transduction concept by which the CEs operate, the question was asked whether in all members of the MGC family they exist in conserved structural motifs.

The answer was in affirmative. In ROS-GC1 the seven CEs are present in motifs: S⁸³³-T⁸³⁹; D⁸⁶⁹-G⁸⁷⁷; D⁸⁷⁸-V⁸⁸²; R⁹²⁵; M⁹⁴²-V⁹⁵²; N⁹⁵³; and A⁹⁵⁵-S⁹⁶⁰. These motifs are conserved in all seven members of the MGC family (Figure 9) and thus, they are termed CEs motifs, CEMs. It is logical to envision that, as in ROS-GC1, these CEMs are, respectively, involved in Mg²⁺ binding, ribose positioning, guanine recognition, and triphosphate angling. We therefore propose that for all MGCs the CEMs control their basal and ligand-dependent catalytic activities.

FIGURE 9

FIGURE 9. Conservation of the seven CEs of CCD in mammalian MGCs. The sequences of the CE modules of bovine ROS-GC1: CEM1, S⁸³³-T⁸³⁹; CEM2, D⁸⁶⁹-G⁸⁷⁷; CEM3, D⁸⁷⁸-V⁸⁸²; CEM4, R⁹²⁵; CEM5, M⁹⁹⁸-V⁹⁵²; CEM6, N⁹⁵³; CEM7, A⁹⁵⁵-S⁹⁶⁰ were aligned with the corresponding sequences of bovine ROS-GC2 (GC-F), rat ONE-GC (GC-D), rat ANF-RGC (NPR-A), human CNP-RGC (NPR-B), human STa-RGC (hSTAR) and rat GC-G. The names in brackets are the alternate names according to NCBI PubMed. Conserved residues are marked in red. The alignment demonstrates total conservation of the CEs and modules they reside in. The CEs are indicated as: predicted to be involved in Mg²⁺ binding (CEM1 and CEM3); guanine recognition (CEM2 and CEM5); predicted to be involved in ribose binding (CEM6); predicted to be involved in triphosphate binding (CEM4 and CEM7).

CCDs of the MGC Family Embody a Conserved ROS-GC1’s 22-Residue Neurocalcin δ (NCδ)–Modulated Structural Domain

Prior to the remarkable discovery that ROS-GC1 CCD is embedded with the residence of neurocalcin δ (NCδ) recognition site (Venkataraman et al., 2008), CCD was believed to be only the translational center of the ligand-dependent signals into the production of cyclic GMP. Linkage with NCδ changed this paradigm, CCD also became a regulatory center for the NCδ-modulated Ca²⁺signals. Strikingly, in contrast to all other ligand-dependent signals, NCδ-modulated Ca²⁺ signal originates and gets transduced in CCD.

To determine if presence of the NCδ-sensing motif, V⁸³⁶-L⁸⁵⁷, is a common feature of the MGC family, sequence of this motif was compared in all members of the MGC family (Figure 10). With 100% conservation, ROS-GC1 and ROS-GC2 preserved this motif and there was about 87% conservation in ONE-GC. With the remainder four MGCs the respective percentile conservation was: ANF-RGC 68; CNP-RGC, 68; Star-GC, 68; and GC-G, 59. In accordance with this pattern, it has been experimentally validated that like ROS-GC1, ONE-GC is Ca²⁺-modulated via its sensor myr-NCδ (Duda et al., 2001; Krishnan et al., 2004; Duda and Sharma, 2008; Sharma and Duda, 2010). Importantly, with the evidence that ANF-RGC also is Ca²⁺- modulated via its sensor myr-NCδ (Duda et al., 2012a) and its NCδ sensing motif has total sequence conservation with the corresponding region in CNP-RGC (Figure 10), we conclude that this motif plays an important physiological role in the regulatory property of the MGC family. Notably, total conservation of the N-terminal VGFT and C-terminal- -LND flanking regions of the NCδ sensing motif is a family trait (Figure 10).

FIGURE 10

FIGURE 10. Sequence alignment of the ROS-GC1 neurocalcin δ binding site with the corresponding regions of other mammalian MGCs. Sequence of ROS-GC1 neurocalcin δ binding site, amino acid residues V⁸³⁶-L⁸⁵⁷, was aligned with the corresponding regions of bovine ROS-GC2 (GC-F), rat ONE-GC (GC-D), rat ANF-RGC (NPR-A), human CNP-RGC (NPR-B), human STa-RGC (hSTAR) and rat GC-G. The names in brackets are the alternate names according to NCBI PubMed. Positions of the amino acid residues of all these MGCs correspond to mature proteins. The conserved residues are marked in red.

CCDs of the MGC Family House Also a Conserved ROS-GC1’s 108-Residue CO₂-Modulated Region

Adding further complexity to the modular role of the CCD, recent studies show that ROS-GC1’s CCD also contains a 108-residue, Y⁸⁵⁸–Y⁹⁶⁵, structural element (Duda et al., 2015, 2016). Except for one residue, Y⁹⁶⁵, it resides within the CCD; and it represents a Ca²⁺-independent CO₂-modulated region of the GC (Figure 1) (Makino et al., 2017). This region shows 70 to 95% identity in the MGC family, is also CO₂-modulated in ONE-GC and possibly in GC-G. Thus, MGC CCD besides containing CEs, contains also two, NCδ and CO₂, modulated regions.

Transmembrane Domain Is a Major Contributor of the MGCs CCD Activity

Right from the time of MGC activity detection in the mammalian tissues the mystery surrounded on one of its features: why, in contrast to the adenylate cyclase which uses Mg²⁺, the preferred cofactor of MGC is Mn²⁺ (Hardman and Sutherland, 1969; Ishikawa et al., 1969; Schultz et al., 1969; White and Aurbach, 1969) (reviewed in Sharma, 2010)?

This mystery has been sustained even with the crystalized forms of the eukaryotic Cyg12 soluble (Winger et al., 2008) and the bacterium Cya2 (Rauch et al., 2008) membrane forms. These CCDs show no significant catalytic activities when the Mg²⁺-GTP substrate is used; they only show these with the use of Mn²⁺-GTP.

To address this issue, we performed domain-by-domain deletion/expression analysis of the recombinant ROS-GC1 (Figure 11). The catalytic activity [pmol cyclic GMP min^-1 (mg prot)^-1] of each truncated construct was assessed using the natural Mg²⁺-GTP as the substrate. The isolated soluble CCD construct contained only a minimal basal specific catalytic activity of 7 pmol. In contrast, the r-ROS-GC1’s basal catalytic activity and of all its truncated constructs ranged between 110 and 130 pmol, a value almost 22-fold higher than its isolated form. Importantly, whenever the constructs lacked the TMD, illustrated by the CCD–CTE and CCD, the CCD’s catalytic activity dramatically dropped from 130 to 6 pmol. To rule out the unlikely possibility that the drop in catalytic activity might be restored by anchoring CCD with any domain located N-terminally to it, the CCD’s catalytic activity was assessed in the partially truncated KHD^--SHD-CCD-CTE soluble fragment (Figure 11). No restoration occurred, however. The catalytic activity remained 6 pmol.

FIGURE 11

FIGURE 11. Transmembrane domain contributes to the ROS-GC1 catalytic activity. The left panel presents schematically various ROS-GC1 deletion mutants. The first five abridged forms of ROS-GC1 have retained TMD whereas the three at the bottom are devoid of TMD thus they are soluble constructs. The membraneous and soluble constructs were prepared and expressed as described in “Materials and Methods” section; the dimerization of the soluble constructs was verified by FPLC as in Venkataraman et al. (2008); for the isolated core catalytic domain mutant (CCD), the ability to form antiparallel homodimer was verified by bifunctional fluorescence (Duda et al., 2012b). They were and assayed for guanylate cyclase activity in the presence of 1 mM GTP and 4 mM Mg²⁺. The right panel provides the values of specific guanylate cyclase activity [pmol cyclic GMP min^-1 (mg prot)^-1] of each construct.

Our interpretation of these results is that: (1) the natural substrate of the MGC’s CCD for catalysis is Mg²⁺-GTP; (2) none of the modular domains- -ExtD, JMD, KHD, SHD and CTE- -have any role in its basic catalytic operation; and (3) TMD is the major contributor in boosting CCD’s basal catalytic activity.

To understand how TMD might contribute to the CCD’s catalytic activity, the possibility was considered that this might be due to a unique consensus motif of the TMDs. Structural comparison, however, demonstrated that this was not the case (Figure 12). Compared to the ROS-GC1, the percentile identity between the MGCs TMDs was only marginal, ROS-GC2, 24; ONE-GC, 24; Star-GC, 22; GC-G, 32; ANF-RGC, 24; CNP-RGC, 25. It is noteworthy that not even a single residue was fully conserved among the family members. Thus, we propose that TMD contributes to the CCD’s catalytic activity by making it possible that all the successive modular domains- -JMD, KHD, SHD, and CCD- are in properly fixed positions (Top Panel: Figure 1), resulting in the optimal conditions for catalysis to occur.

FIGURE 12

FIGURE 12. Sequence comparison of mammalian MGCs TMD. The sequences of TMDs of bovine ROS-GC1 (GC-E), bovine ROS-GC2 (GC-F), rat ONE-GC (GC-D), rat ANF-RGC (NPR-A), human CNP-RGC (NPR-B), human STa-RGC (hSTAR) and rat GC-G were aligned. The names in brackets are alternate names according to NCBI PubMed. Positions of the amino acid residues of all these MGCs correspond to mature proteins. The conserved amino acid residues are marked in red.

Discussion

Using the model system of photoreceptor ROS-GC1 the presented study (a) decodes the basic structure and biochemistry of the core unit of CCD; (b) models its three-dimensional configuration; (c) develops a general MGC family signal transduction theme; and (d) experimentally validates the theme for ROS-GC1.

Basic Structure

Encoded by seven genes, MGC is the generator of cyclic GMP which serves as an intracellular second messenger for the countless physiological processes. It is a single transmembrane spanning protein existing as a homodimer upheld by two contact regions between the monomers (Figure 1). Based on the crystal structure of the ANF-RGC ExtD (Ogawa et al., 2004), the first prototype guanylate cyclase member (reviewed in Sharma et al., 2016), there is head-to-head contact of these two domains. The second contact is formed at the CCD (Venkataraman et al., 2008) where two monomers assume an antiparallel conformation (Duda et al., 2012b) and (Figure 1). The encoded seven MGCs- -ANF-RGC, CNP-RGC, STa-RGC, ROS-GC1, ROS-GC2, ONE-GC and GC-G- -initiate cellular signaling process from different sites, the first three from the ExtD, next two from the ICD, ONE-GC from both ExtD and ICD and GC-GC, most probably from ICD (Sharma et al., 2016). Yet, regardless of the origin, all signals are transduced and translated into the generation of cyclic GMP at the CCD (Sharma et al., 2016).

Three-Dimensional Model

In the photoreceptor ROS-GC1, a mammalian MGC, CCD is a 145-residue structural unit stretching from V⁸²⁰ to P⁹⁶⁴ (Figure 1). In its natural form, it is homodimeric. In its simulated 3D-model, each monomer is composed of 8-stranded β-sheets and six α-helices (Figure 3A). In its homodimer form two monomers assume a two-fold symmetry axis with a central gap of a circlet-like shape (Figure 3B). The circlet between the monomers contains two symmetric active sites, each formed by the conserved residues (CEs) from the two monomers (Figure 3C). The CEs are: two Mg²⁺-binding, D⁸³⁴ and D⁸⁷⁸; one, ribose positioning, N⁹⁵³; two guanine recognition, E⁸⁷⁴ and C⁹⁴⁶; and two, triphosphate angling, R⁹²⁵ and R⁹⁵⁷. The projection is that in an inactive state the dimer is in an open conformation but in closed upon binding GTP for catalysis (Figure 3D).

General Signal Transduction Theme

The CCD structure is conserved in all seven mammalian MGCs, showing a sequence identity between 92 and 65% (Figure 8). Characteristically, it is closer between the Ca²⁺-modulated guanylate cyclases – -compare ROS-GC1 vs ROS-GC2, 93% and ROS-GC1 vs ONE-GC, 85%. It is predicted that this closeness in identity is reflective of the regulatory feature of the CCD, in contrast to its basic catalytic mode, explained below.

In a uniform general mode, all seven CEs of all MGCs are arranged in structural motifs (Figure 9). These motifs, respectively, represent the common features of all MGCs. This structured theme of the motifs points out that they in an identical fashion control the folding patterns of all MGCs and, thus, their basic guanylate cyclase catalytic activities.

The presented study also discloses two important features of the mammalian MGC CCD.

(1) An extraordinary characteristic that sets the mammalian MGC family apart from the soluble (Winger et al., 2008) and the bacterium MGC (Rauch et al., 2008) is that the mammalian CCD uses natural Mg²⁺-GTP as a substrate for catalysis. It is understandable for the bacterium MGC’s CCD to use Mn²⁺-GTP because bacteria need this trace element for survival. Yet, it is surprising in the case of eukaryotic soluble guanylate cyclase, Cyg12, because this cation is not its natural substrate for catalysis.

(2) To this moment, it has been a mystery as to why the basal catalytic activity of the MGC CCD drops about 90% in its’ isolated from. In a major contribution, this study solves this riddle. The solution resides in its TMD. The TMD anchors it, fixes its conformation and makes it more amenable to the signal transduction events involved in controlling its basal and catalytic events. Importantly, the possibility that this characteristic might be due to a unique signaling characteristic of a structural element in the TMD has been ruled out because such an element does not exist in TMD (Figure 12).

Predictions, Experimentally Validated

In accordance with the predictions, (i) MGC CCD is homo-dimeric. (ii) Seven CEs embedded in their seven CE motifs, all are critical in controlling the basal catalytic activity of the MGCs. (iii) Mg²⁺-GTP is the natural substrate for catalysis, this basic operation is controlled by the CEM motifs, 2 and 3. (iv) The TM domain by anchoring MGC to the plasma membrane controls almost all (more than 90%) the basal CCD activity. (v) Besides its core seven-CE elemental structure, the catalytic domain is embedded with two regulatory domains, NCδ and CO₂; thus, CCD is both a core and regulatory catalytic center. (vi) CCD controls all four phototransduction pathways (discussed below).

Photoreceptor ROS-GC1 Linkage with Phototransduction

Similar to its critical role in controlling the basic catalytic operation of the MGC family, CCD also plays a vital regulatory role in modulating all four ROS-GC1 interlocked phototransduction pathways. The mutation in any one of its seven CE elements severely impedes it’s all Ca²⁺-modulated rod and cone photoreceptor along with the Ca²⁺-modulated and CO₂/bicarbonate-modulated catalytic activity. The cyclic GMP output in the cells is compromised, and it is predicted that finally the photoreceptors will die. Notably, the ligand-modulated EC₅₀ and Hill coefficient values of the pathways are not affected, demonstrating that CEs core element has no control over the ligand binding activities of the ROS-GC.

Model

The MGC signal transduction is a two-step process. Step one, it is contributed by the seven CE elements of the CCD and occurs in all members of the MGC family. The CCD captures Mg²⁺-GTP in its pocket and turns itself from the inactive basal to the active basal state (Figure 3D). Step two, it is a regulatory process. Upon ligand (GCAP1, GCAP2, S100B, or bicarbonate) binding, the rotation of each CCD monomer occurs around their two-fold axes (Figure 3C). This brings the CE residues into the closed maximally active position, and collectively their manifestation of the ligand dependent catalytic saturation activity.

Conclusion

This study has predicted and experimentally solved the basic 3D-structure of the CCD existing in all members of the MGC family, demonstrated a unified code by which it operates; and, then applied this knowledge to explain some of the most fundamental principles by which the ROS-GC1 is interlocked with phototransduction in rods and cones. Finally and strikingly, the existing seven MGCs—ANF-RGC, CNP-RGC, STa-RGC, ROS-GC1, ROS-GC2, ONE-GC, GC-GC—in a specific fashion, by synthesizing cellular second messenger cyclic GMP, are linked with the physiological processes of blood pressure regulation, cellular growth, sensory transductions, neural plasticity, memory, temperature sensing (reviewed in Sharma et al., 2016) and, with tumor suppression (reviewed in Steinbrecher and Cohen, 2011; Windham and Tinsley, 2015). This study demonstrates that all these functions converge to a common site, CCD, which through a unified signal transduction mode, control these activities.

Author Contributions

TD designed, carried out the experiments and analyzed their results. SR created and explained the stereo models. AP created and expressed all the mutants. RS conceptually planned and coordinated the study and sided in generating the model. All authors contributed to the writing of the manuscript.

Funding

This work was supported in by the National Eye Institute: EY 023980 and with federal funds from the National Cancer Institute, National Institutes of Health, under contract HHSN 261200800001E. The authors are solely responsible for the contents of this study, which may not represent the official views of the National Institutes of Health or policies of the Department of Health and Human Services. There is no mention of trade names, commercial products, or organizations implying endorsement by the US government.

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.

Acknowledgment

We thank Dr. Clint Makino, Boston University, for constructive comments on the manuscript.

Supplementary Material

The Supplementary Material for this article can be found online at: http://journal.frontiersin.org/article/10.3389/fnmol.2017.00173/full#supplementary-material

Footnotes

1. ^ http://zhanglab.ccmb.med.umich.edu/I-TASSER/
2. ^ http://fatcat.sanfordburnham.org/

References

Anantharaman, V., Balaji, S., and Aravind, L. (2006). The signaling helix: a common functional theme in diverse signaling proteins. Biol. Direct 1:25. doi: 10.1186/1745-6150-1-25

PubMed Abstract | CrossRef Full Text | Google Scholar

Chang, M. S., Lowe, D. G., Lewis, M., Hellmiss, R., Chen, E., and Goeddel, D. V. (1989). Differential activation by atrial and brain natriuretic peptides of two different receptor guanylate cyclases. Nature 341, 68–72. doi: 10.1038/341068a0

PubMed Abstract | CrossRef Full Text | Google Scholar

Chinkers, M., and Garbers, D. L. (1989). The protein kinase domain of the ANP receptor is required for signaling. Science 245, 1392–1394. doi: 10.1126/science.2571188

CrossRef Full Text | Google Scholar

Chinkers, M., Garbers, D. L., Chang, M. S., Lowe, D. G., Chin, H. M., Goeddel, D. V., et al. (1989). A membrane form of guanylate cyclase is an atrial natriuretic peptide receptor. Nature 338, 78–83. doi: 10.1038/338078a0

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Fik-Rymarkiewicz, E., Venkataraman, V., Krishnan, R., Koch, K. W., and Sharma, R. K. (2005). The calcium-sensor guanylate cyclase activating protein type 2 specific site in rod outer segment membrane guanylate cyclase type 1. Biochemistry 44, 7336–7345. doi: 10.1021/bi050068x

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Goraczniak, R. M., and Sharma, R. K. (1991). Site-directed mutational analysis of a membrane guanylate cyclase cDNA reveals the atrial natriuretic factor signaling site. Proc. Natl. Acad. Sci. U.S.A. 88, 7882–7886. doi: 10.1073/pnas.88.17.7882

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Jankowska, A., Venkataraman, V., Nagele, R. G., and Sharma, R. K. (2001). A novel calcium-regulated membrane guanylate cyclase transduction system in the olfactory neuroepithelium. Biochemistry 40, 12067–12077. doi: 10.1021/bi0108406

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Koch, K. W., Venkataraman, V., Lange, C., Beyermann, M., and Sharma, R. K. (2002). Ca²⁺ sensor S100beta-modulated sites of membrane guanylate cyclase in the photoreceptor-bipolar synapse. EMBO J. 21, 2547–2556. doi: 10.1093/emboj/21.11.2547

CrossRef Full Text | Google Scholar

Duda, T., Pertzev, A., Makino, C. L., and Sharma, R. K. (2016). Bicarbonate and Ca²⁺ sensing modulators activate photoreceptor ROS-GC1 synergistically. Front. Mol. Neurosci. 9:5. doi: 10.3389/fnmol.2016.00005

CrossRef Full Text | Google Scholar

Duda, T., Pertzev, A., and Sharma, R. K. (2011). 657WTAPELL663 motif of the photoreceptor ROS-GC1: a general phototransduction switch. Biochem. Biophys. Res. Commun. 408, 236–241. doi: 10.1016/j.bbrc.2011.03.134

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Pertzev, A., and Sharma, R. K. (2012a). Ca²⁺ modulation of ANF-RGC: new signaling paradigm interlocked with blood pressure regulation. Biochemistry 51, 9394–9405. doi: 10.1021/bi301176c

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Pertzev, A., and Sharma, R. K. (2012b). Differential Ca²⁺ sensor guanylate cyclase activating protein modes of photoreceptor rod outer segment membrane guanylate cyclase signaling. Biochemistry 51, 4650–4657. doi: 10.1021/bi300572w

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., and Sharma, R. K. (2008). ONE-GC membrane guanylate cyclase, a trimodal odorant signal transducer. Biochem. Biophys. Res. Commun. 367, 440–445. doi: 10.1016/j.bbrc.2007.12.153

PubMed Abstract | CrossRef Full Text | Google Scholar

Duda, T., Wen, X. H., Isayama, T., Sharma, R. K., and Makino, C. L. (2015). Bicarbonate modulates photoreceptor guanylate cyclase (ROS-GC) catalytic activity. J. Biol. Chem. 290, 11052–11060. doi: 10.1074/jbc.M115.650408

PubMed Abstract | CrossRef Full Text | Google Scholar

Garbers, D. L. (1992). Guanylyl cyclase receptors and their endocrine, paracrine, and autocrine ligands. Cell 71, 1–4. doi: 10.1016/0092-8674(92)90258-E

CrossRef Full Text | Google Scholar

Goraczniak, R. M., Duda, T., Sitaramayya, A., and Sharma, R. K. (1994). Structural and functional characterization of the rod outer segment membrane guanylate cyclase. Biochem. J. 302(Pt 2), 455–461. doi: 10.1042/bj3020455

CrossRef Full Text | Google Scholar

Hardman, J. G., and Sutherland, E. W. (1969). Guanyl cyclase, an enzyme catalyzing the formation of guanosine 3′,5′-monophosphate from guanosine triphosphate. J. Biol. Chem. 244, 6363–6370.

Google Scholar

Ishikawa, E., Ishikawa, S., Davis, J. W., and Sutherland, E. W. (1969). Determination of guanosine 3′,5′-monophosphate in tissues and of guanyl cyclase in rat intestine. J. Biol. Chem. 244, 6371–6376.

Google Scholar

Koch, K. W., and Dell’orco, D. (2013). A calcium-relay mechanism in vertebrate phototransduction. ACS Chem. Neurosci. 4, 909–917. doi: 10.1021/cn400027z

PubMed Abstract | CrossRef Full Text | Google Scholar

Krishnan, A., Venkataraman, V., Fik-Rymarkiewicz, E., Duda, T., and Sharma, R. K. (2004). Structural, biochemical, and functional characterization of the calcium sensor neurocalcin delta in the inner retinal neurons and its linkage with the rod outer segment membrane guanylate cyclase transduction system. Biochemistry 43, 2708–2723. doi: 10.1021/bi035631v

PubMed Abstract | CrossRef Full Text | Google Scholar

Kumar, V. D., Vijay-Kumar, S., Krishnan, A., Duda, T., and Sharma, R. K. (1999). A second calcium regulator of rod outer segment membrane guanylate cyclase, ROS-GC1: neurocalcin. Biochemistry 38, 12614–12620. doi: 10.1021/bi990851n

PubMed Abstract | CrossRef Full Text | Google Scholar

Liu, Y., Ruoho, A. E., Rao, V. D., and Hurley, J. H. (1997). Catalytic mechanism of the adenylyl and guanylyl cyclases: modeling and mutational analysis. Proc. Natl. Acad. Sci. U.S.A. 94, 13414–13419. doi: 10.1073/pnas.94.25.13414

PubMed Abstract | CrossRef Full Text | Google Scholar

Lowe, D. G., Chang, M. S., Hellmiss, R., Chen, E., Singh, S., Garbers, D. L., et al. (1989). Human atrial natriuretic peptide receptor defines a new paradigm for second messenger signal transduction. EMBO J. 8, 1377–1384.

PubMed Abstract | Google Scholar

Makino, C. L., Pertzev, A., Sharma, R. K., and Duda, T. (2017). “Bicarbonate enters a rod thru its synapse to stimulate ROS-GC in its outer segment, whereas cones generate bicarbonate intracellularly from CO₂,” in Proceedings of the ARVO 2017 Annual Meeting Abstracts, Rockville, MD.

Makino, C. L., Peshenko, I. V., Wen, X. H., Olshevskaya, E. V., Barrett, R., and Dizhoor, A. M. (2008). A role for GCAP2 in regulating the photoresponse. Guanylyl cyclase activation and rod electrophysiology in GUCA1B knock-out mice. J. Biol. Chem. 283, 29135–29143. doi: 10.1074/jbc.M804445200

PubMed Abstract | CrossRef Full Text | Google Scholar

Makino, C. L., Wen, X. H., Olshevskaya, E. V., Peshenko, I. V., Savchenko, A. B., and Dizhoor, A. M. (2012). Enzymatic relay mechanism stimulates cyclic GMP synthesis in rod photoresponse: biochemical and physiological study in guanylyl cyclase activating protein 1 knockout mice. PLoS ONE 7:e47637. doi: 10.1371/journal.pone.0047637

PubMed Abstract | CrossRef Full Text | Google Scholar

Nambi, P., Aiyar, N. V., Roberts, A. N., and Sharma, R. K. (1982). Relationship of calcium and membrane guanylate cyclase in adrenocorticotropin-induced steroidogenesis. Endocrinology 111, 196–200. doi: 10.1210/endo-111-1-196

PubMed Abstract | CrossRef Full Text | Google Scholar

Ogawa, H., Qiu, Y., Ogata, C. M., and Misono, K. S. (2004). Crystal structure of hormone-bound atrial natriuretic peptide receptor extracellular domain: rotation mechanism for transmembrane signal transduction. J. Biol. Chem. 279, 28625–28631. doi: 10.1074/jbc.M313222200

PubMed Abstract | CrossRef Full Text | Google Scholar

Paul, A. K., Marala, R. B., Jaiswal, R. K., and Sharma, R. K. (1987). Coexistence of guanylate cyclase and atrial natriuretic factor receptor in a 180-kD protein. Science 235, 1224–1226. doi: 10.1126/science.2881352

PubMed Abstract | CrossRef Full Text | Google Scholar

Pozdnyakov, N., Goraczniak, R., Margulis, A., Duda, T., Sharma, R. K., Yoshida, A., et al. (1997). Structural and functional characterization of retinal calcium-dependent guanylate cyclase activator protein (CD-GCAP): identity with S100beta protein. Biochemistry 36, 14159–14166. doi: 10.1021/bi971792l

PubMed Abstract | CrossRef Full Text | Google Scholar

Ramamurthy, V., Tucker, C., Wilkie, S. E., Daggett, V., Hunt, D. M., and Hurley, J. B. (2001). Interactions within the coiled-coil domain of RetGC-1 guanylyl cyclase are optimized for regulation rather than for high affinity. J. Biol. Chem. 276, 26218–26229. doi: 10.1074/jbc.M010495200

PubMed Abstract | CrossRef Full Text | Google Scholar

Rauch, A., Leipelt, M., Russwurm, M., and Steegborn, C. (2008). Crystal structure of the guanylyl cyclase Cya2. Proc. Natl. Acad. Sci. U.S.A. 105, 15720–15725. doi: 10.1073/pnas.0808473105

PubMed Abstract | CrossRef Full Text | Google Scholar

Saha, S., Biswas, K. H., Kondapalli, C., Isloor, N., and Visweswariah, S. S. (2009). The linker region in receptor guanylyl cyclases is a key regulatory module: mutational analysis of guanylyl cyclase C. J. Biol. Chem. 284, 27135–27145. doi: 10.1074/jbc.M109.020032

PubMed Abstract | CrossRef Full Text | Google Scholar

Sambrook, J., Fritsch, E. F., and Maniatis, T. (eds) (1989). “Expression of cloned genes in cultured mammalian cells,” in A Laboratory Manual, 2nd Edn, (Cold Spring Harbor, NY: Cold Spring Harbor Laboratory), 16.11–16.81.

Google Scholar

Schultz, G., Bohme, E., and Munske, K. (1969). Guanyl cyclase. Determination of enzyme activity. Life Sci. 8, 1323–1332. doi: 10.1016/0024-3205(69)90189-1

CrossRef Full Text | Google Scholar

Sharma, R. K. (2002). Evolution of the membrane guanylate cyclase transduction system. Mol. Cell. Biochem. 230, 3–30. doi: 10.1023/A:1014280410459

CrossRef Full Text | Google Scholar

Sharma, R. K. (2010). Membrane guanylate cyclase is a beautiful signal transduction machine: overview. Mol. Cell. Biochem. 334, 3–36. doi: 10.1007/s11010-009-0336-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Sharma, R. K., and Duda, T. (2010). Odorant-linked ROS-GC subfamily membrane guanylate cyclase transduction system. Mol. Cell. Biochem. 334, 181–189. doi: 10.1007/s11010-009-0333-9

PubMed Abstract | CrossRef Full Text | Google Scholar

Sharma, R. K., and Duda, T. (2014). Membrane guanylate cyclase, a multimodal transduction machine: history, present, and future directions. Front. Mol. Neurosci. 7:56. doi: 10.3389/fnmol.2014.00056

PubMed Abstract | CrossRef Full Text | Google Scholar

Sharma, R. K., Duda, T., and Makino, C. L. (2016). Integrative signaling networks of membrane guanylate cyclases: biochemistry and physiology. Front. Mol. Neurosci. 9:83. doi: 10.3389/fnmol.2016.00083

PubMed Abstract | CrossRef Full Text | Google Scholar

Sharma, R. K., Makino, C. L., Hicks, D., and Duda, T. (2014). ROS-GC interlocked Ca²⁺-sensor S100B protein signaling in cone photoreceptors: review. Front. Mol. Neurosci. 7:21. doi: 10.3389/fnmol.2014.00021

CrossRef Full Text | Google Scholar

Shyjan, A. W., de Sauvage, F. J., Gillett, N. A., Goeddel, D. V., and Lowe, D. G. (1992). Molecular cloning of a retina-specific membrane guanylyl cyclase. Neuron 9, 727–737. doi: 10.1016/0896-6273(92)90035-C

CrossRef Full Text | Google Scholar

Steinbrecher, K. A., and Cohen, M. B. (2011). Transmembrane guanylate cyclase in intestinal pathophysiology. Curr. Opin. Gastroenterol. 27, 139–145. doi: 10.1097/MOG.0b013e328341ead5

PubMed Abstract | CrossRef Full Text | Google Scholar

Sunahara, R. K., Tesmer, J. J., Gilman, A. G., and Sprang, S. R. (1997). Crystal structure of the adenylyl cyclase activator Gsalpha. Science 278, 1943–1947. doi: 10.1126/science.278.5345.1943

PubMed Abstract | CrossRef Full Text | Google Scholar

Tucker, C. L., Hurley, J. H., Miller, T. R., and Hurley, J. B. (1998). Two amino acid substitutions convert a guanylyl cyclase, RetGC-1, into an adenylyl cyclase. Proc. Natl. Acad. Sci. U.S.A. 95, 5993–5997. doi: 10.1073/pnas.95.11.5993

PubMed Abstract | CrossRef Full Text | Google Scholar

Venkataraman, V., Duda, T., Ravichandran, S., and Sharma, R. K. (2008). Neurocalcin delta modulation of ROS-GC1, a new model of Ca²⁺ signaling. Biochemistry 47, 6590–6601. doi: 10.1021/bi800394s

PubMed Abstract | CrossRef Full Text | Google Scholar

Wen, X. H., Duda, T., Pertzev, A., Venkataraman, V., Makino, C. L., and Sharma, R. K. (2012). S100B serves as a Ca²⁺ sensor for ROS-GC1 guanylate cyclase in cones but not in rods of the murine retina. Cell Physiol. Biochem. 29, 417–430. doi: 10.1159/000338496

PubMed Abstract | CrossRef Full Text | Google Scholar

White, A. A., and Aurbach, G. D. (1969). Detection of guanyl cyclase in mammalian tissues. Biochim. Biophys. Acta 191, 686–697. doi: 10.1016/0005-2744(69)90362-3

CrossRef Full Text | Google Scholar

Wilson, E. M., and Chinkers, M. (1995). Identification of sequences mediating guanylyl cyclase dimerization. Biochemistry 34, 4696–4701. doi: 10.1021/bi00014a025

PubMed Abstract | CrossRef Full Text | Google Scholar

Windham, P. F., and Tinsley, H. N. (2015). cGMP signaling as a target for the prevention and treatment of breast cancer. Semin. Cancer Biol. 31, 106–110. doi: 10.1016/j.semcancer.2014.06.006

PubMed Abstract | CrossRef Full Text | Google Scholar

Winger, J. A., Derbyshire, E. R., Lamers, M. H., Marletta, M. A., and Kuriyan, J. (2008). The crystal structure of the catalytic domain of a eukaryotic guanylate cyclase. BMC Struct. Biol. 8:42. doi: 10.1186/1472-6807-8-42

PubMed Abstract | CrossRef Full Text | Google Scholar