M.
Raja‡
a,
T.
Puntheeranurak‡
b,
H. J.
Gruber
c,
P.
Hinterdorfer
c and
R. K. H.
Kinne
*a
aMax Planck Institute of Molecular Physiology, Dortmund, Germany. E-mail: rolf.kinne@mpi-dortmund.mpg.de
bDepartment of Biology, Center of Nanoscience, Faculty of Science, Mahidol University, Ratchathevi, Bangkok, Thailand
cInstitute for Biophysics, Christian Doppler Laboratory of Nanoscopic Methods in Biophysics, Johannes Kepler University of Linz and Center for Advanced Bioanalysis GmbH (CBL), Linz, Austria
First published on 15th April 2016
This article reviews the role of segments of SLCs located outside the plasma membrane bilayer (ectodomains) using the inhibition of SGLTs (SLC5 family) by the aromatic glucoside phlorizin as a model system. Phlorizin has been the lead substance for the development of SGLT2 (SLC5A2) inhibitors that have been introduced recently for the treatment of type 2 diabetes. Using mainly biophysical methods, it is shown that three ectodomains form well-defined substructures, such as short helices, that are arranged in a vestibule and undergo significant conformational changes during binding of phlorizin. From these data, tentative structures of inhibitor/ectodomain complexes are derived by molecular modeling. The ectodomains provide an additional binding site for aglucones, which cooperates with the binding site for the sugar moiety of phlorizin in the sugar translocation pathway, buried inside the membrane. They play a significant role in determining the specificity, selectivity, and affinity of sugar transport inhibitors and might even explain the difference in sensitivity of various members of the SGLT family, located in different tissues and organs of the human body. Similar binding modes are suggested for several other SLCs, in particular the monoamine transporter (SLC6 family), that belong to the sodium/neurotransmitter cotransporter family.
Detailed information at the molecular level is now available for almost all transporters. It is derived mostly from X-ray analysis of transporter molecules crystallized in outward-facing, occluded or inward-facing configurations combined with studies in which putative substrate binding sites have been mutated. Due to the complex structures of membrane proteins, these studies describe mostly those parts which are embedded in the phospholipid bilayer (endodomains) and can be captured in the “frozen” state of a crystal. However, the parts of transporters outside the membrane (ectodomains) can rarely be resolved because of their high flexibility and inherent mobility. Recently, molecular modelling studies on drug binding and specificity8–10 as well as single molecule recognition and force spectroscopy studies by atomic force microcopy (AFM)11–14 have revealed the importance of vestibules formed by extramembranous loops on the cell surface in target recognition, in defining drug specificity and in governing binding processes. The overall idea of exploiting ectodomain–ligand interactions to achieve target specificity and enhanced binding affinity is a novel potential general strategy for inhibitor/drug development.
The current review summarizes the information available on the role of extracellular ectodomains in the interaction of inhibitors with SLCs. It focuses mainly on the inhibitory action of phlorizin, a glucoside and the leading substance for developing SGLT2 inhibitors. The data obtained in single molecule analysis by AFM on intact cells and in studies of isolated ectodomains in solution are used to model the SGLT–inhibitor interactions. Investigations on other SLCs, in particular SERT (SLC6A4), are briefly mentioned in which homology modeling, induced fit docking calculation, and molecular dynamics simulation combined with site directed mutagenesis also suggest potential interactions of inhibitors with ectodomains. These studies complement, enrich and deepen our knowledge on drug–target interactions and may provide new tools for the development of drugs targeting specifically biologically important membrane transporters.
SGLT2 is responsible for bulk reabsorption of D-glucose from the primary urine in early parts of the renal proximal tubule, and the residual sugar is almost completely removed by SGLT1 in the late proximal tubule.15 Isoforms SGLT3 to SGLT5 have been found in a variety of other tissues (for a complete list, see ref. 5). In functional studies, SGLT1 and SGLT2 have been found to be inhibited by aromatic glucosides. The most extensively studied glucoside is phlorizin in which D-glucose is linked to the aglucone phloretin via a beta-glycosidic bond (see Fig. 1 for chemical structures). In addition, alkyl-glucosides inhibit the transporter (see Fig. 1 for chemical structures).16
SGLT2 has recently been identified as a target for the treatment of diabetes;3 based on phlorizin as the leading substance, drugs such as canagliflozin and dapagliflozin (see Fig. 1 for chemical structures) have been developed and introduced into the market.4 Another exciting discovery was that some pancreatic and prostatic cancer cells express SGLT2 and their metabolism and growth depend on the uptake of D-glucose via this transport pathway, suggesting the possibility for an effective treatment.17 Kinetic studies on intact cells or plasma membranes have shown that phlorizin and other SGLT2 inhibitors act from the extracellular side.18,19 The interaction of phlorizin with the SGLT transporter involves the sugar-binding site of the transporter and aglucone-binding sites.20 The affinity of SGLT1 for phlorizin is about 1000-fold higher than that for glucose.21
A bacterial homologue of SGLT has been crystallized, and its structure has been determined. The model proposed for the translocation of sugars, integrating kinetic and structural data, contains the following steps.7 First, Na+ binds to the ligand-free outside-facing state of the transporter to open the outward-facing gate, permitting outside sugar to bind and be subsequently trapped in the substrate binding site of the transporter in an occluded state, where egress to the outside solution is blocked. This is followed by a conformational change from the outward-occluded state to an inward-occluded state. On opening the inward gate, the Na+ ions and sugar are released into the cell interior. The transport cycle is completed by the change in conformation from the inward-facing ligand-free state to the outward-facing ligand-free state.
Structural and biophysical data predict that formation of the phlorizin–SGLT complex creates an additional, highly condensed conformational state which makes translocation of sugars impossible.20,22 The bacterial sodium glucose cotransporter is not inhibited by phlorizin, and until now, no phlorizin–SGLT complex has been crystallized; however, several biochemical, genetic and biophysical studies have been performed. The following sections will summarize the information currently available on phlorizin binding sites, in particular on the ectodomains of the SGLT transporter facing the outside of glucose transporting cells.
Fig. 2 Schematic representation of an atomic force microscopy force–distance cycle. The tip is moved toward the surface of the cells grown on a flat support (dotted line, 1–2) and subsequently retracted (solid line) at a constant lateral position. If during the approach the ligand attached to the cantilever interacted with a specific binding site on the surface of the cell, during retraction a force signal of a distinct shape (3) (representing a deflection of the cantilever) is observed. The force increases until dissociation occurs (4) at an unbinding force fu. For further details, see ref. 25. |
In a “force–distance cycle”, the cantilever tip tethered with the ligand is first approached towards the surface whereupon a single receptor–ligand complex is formed based on the specific ligand–receptor recognition. Subsequently, the cantilever is retracted from the surface. An increasing bending force is exerted on the cantilever due to the ligand–receptor connection until the interaction bonds break at a critical force (the so-called unbinding force, fu, calculated by using Hooke's law: F = kΔx, where k is the spring constant of the cantilever, and Δx is the cantilever deflection). From such experiments, the specifics of the ligand–receptor interaction such as affinity, binding, unbinding rate constants, and structure of the binding pocket can be delineated (see below).
Various methods to firmly attach ligands at a low surface density to cantilever tips are depicted in Fig. 3.
Fig. 3 Linkage of ligands to AFM cantilever tips. (A) Specific antibodies were covalently coupled to AFM tips via heterobifunctional polyethylene glycol (PEG) linkers, PDP–PEG800–NHS (left) and aldehyde–PEG800–NHS (right). (B) Sugars were covalently linked to AFM tips via vinyl sulfone–PEG800–NHS (large end group) or acrylamide–PEG800 and PEG5000–NHS (small end groups). (C) Maleimide–PEG800–NHS was used to couple phlorizin to AFM tips. In all instances, the NHS ends of the PEG linkers were covalently bound to amines on the functionalized cantilever tips. Abbreviations: PDP = 2-pyridyldithiopropionyl residue, NHS = N-hydroxy-succinimidyl residue.25 |
In order to provide the flexibility of ligands required to interact with complementary macromolecules, a long poly(ethylene glycol) (PEG) chain is inserted between the tip and the probe molecule. PEG is a water soluble, non-toxic, and chemically and physically inert polymer. The PEG linker can vary in length. We commonly use a PEG linker of an extended length of 6 nm; however, longer cross linkers are also available to probe deeper into proteins.24 To construct AFM-tip sensors, the cross linker contains two different functional groups at its ends, i.e. one end couples to the tip of the cantilever and the other to the ligand. Various heterobifunctional cross linkers have been developed. In our laboratory, the cross linker widely used for antibody coupling has an N-hydroxy-succinimidyl (NHS) residue on one end, which reacts to amines on the ethanolamine coated cantilever tip and a 2-pyridyldithiopropionyl (PDP) residue on the other end, which can covalently bind to thiols of proteins (Fig. 3A). This sulfur chemistry is highly advantageous, since it is very reactive and renders site-directed coupling possible. If no free thiols for coupling are available on the native ligands, they can be generated by modification with SATP [N-succinimidyl-3-(S-acetylthio)propionate]. Another linker widely used for protein coupling in our laboratory is aldehyde–PEG800–NHS which interacts with free amino groups of peptide chains28 (Fig. 3A).
Glucose tethered cantilevers were created by using thioglucose, vinyl sulfone–PEG800–NHS, acrylamide–PEG800–NHS or acrylamide–PEG5000–NHS (Fig. 3B). In this AFM tip sensor, the OH groups known to be essential for translocation of D-glucose (i.e. at C2, C3, and C4) were not modified. Maleimide–PEG800–NHS was employed to couple a modified phlorizin to cantilever tips (Fig. 3C). In the following sections, we will describe how these specific AFM cantilevers can be used as biosensors to explore the topology and dynamics of ectodomains, such as conformational changes and substrate–transporter and inhibitor–transporter interactions of the SGLT1 protein in living cells at the single molecule level.
Fig. 4 Recognition of ectodomains of SGLT1 on the surface of intact cells. AFM cantilever tips were tagged with epitope-specific antibodies against subdomain I = PAN 2-2 = loop 7, subdomain II = QUIS 30 = loop 9, and subdomain III = PAN 3-2 = late loop 13 of rbSGLT1 (rabbit isoform of SGLT1). Quantitative comparison of binding probabilities to cells expressing rbSGLT1 in the absence or presence of free specific antibodies in the medium. Triple asterix indicate statistical significance, for further details see ref. 25. |
Specificity of recognition was confirmed in “blocking experiments”, either by saturating the surface of cells with free antibodies against SGLT or by blocking antibodies attached to the AFM tip with free antigens. Thereby, recognition events disappeared (Fig. 4) and the force–distance cycles were similar to the ones obtained from non-expressing cells (data not shown). To achieve statistical significance, up to 500–1000 force–distance cycles were performed for each location on the surface of cells, and up to four locations (different cells) were investigated for each condition. Thus, it could be demonstrated, at the molecular level, that these three ectodomains of SGLT1 can be specifically recognized on the surface of living cells by epitope-specific antibodies. This provides strong evidence that they are located on the outer membrane surface of the transporter. Interestingly, our results also show that at least the late part of subdomain III is accessible from the extracellular space, suggesting a model for the membrane topology of the transporter shown in Fig. 5, which contains a membrane-crossing loop between TMH 13 and 14.
Fig. 5 Membrane topology of SGLT1. Three ectodomains (subdomains I to III) are exposed to the extracellular medium; the dotted lines represent the epitopes of the specific antibodies. They are connected by S–S bonds (not shown) and form a vestibule in the access pathway of D-glucose to the translocation site of SGLT1.23 |
Furthermore, transport studies with cysteine mutants suggested the presence of a disulfide bridge between Cys255 in subdomain I and Cys608 in subdomain III. This bridge brings subdomain II in close vicinity to the other subdomains creating a vestibule for initial sugar binding to the transporter. This initial binding reaction studied with AFM-thioglucose exhibits a different stereo-specificity than that found in transport studies, suggesting several consecutive selectivity filters of the transporter (for details see below).23
Fig. 6 Dose–response curves of phlorizin inhibition of sodium-dependent AMG uptake into cells mutated in loop 13. COS 7 cells were transiently transfected with plasmids of rbSGLT1 (WT) or various mutants of SGLT1, in which lysine (K) had been introduced at different sites of subdomain III. AMG uptake into cells was measured in the presence of 5 mmol l−1 alpha-methyl-D-glucopyranoside with or without 120 mM NaCl. Uptake in the presence of various phlorizin concentrations was compared to the uptake in the absence of phlorizin set as 100%.33 |
In all mutants, the apparent affinity of sugar uptake for AMG was not statistically different from that of the wild type. These studies suggest that the region of subdomain III between amino acids 604 and 610 is involved in the interaction between SGLT1 and phlorizin, probably by providing a hydrophobic pocket for one of the aromatic rings of the aglucone moiety of the glycoside.33
Fig. 7 D-Glucose recognition and phlorizin-binding sites in isolated hSGLT1 (human isoform of SGLT1) incorporated in proteoliposomes. The hypothetical scheme of major interaction sites between phlorizin and hSGLT1. The sugar moiety of phlorizin interacts with residues Gln457 and Thr460 present in transmembrane helix IX probably by the same hydrogen bond interactions as D-glucose does; the aromatic rings A and B of the aglucone interact with Phe609/Phe602 in subdomain III.34 |
Thereby, in the phlorizin–carrier complex, a close vicinity between these two subdomains of the transporter is established, creating a phlorizin binding pocket with the previously estimated dimensions of 10 × 17 × 7 Å.20,35,36
The results illustrated in Fig. 8 show that specific unbinding events of 1-thio-glucose to the SGLT1 transporter can be detected only in the presence of sodium. By constructing an empirical probability density function (pdf) of the unbinding force, the maximum of the distribution was found to be about 40–50 pN (Fig. 8B) which was smaller than that obtained with the antibodies. This may due to a lower affinity of the sugar to SGLT1. Moreover, binding events were only detected in CHO cells overexpressing rbSGLT1.
Fig. 8 Interaction of glucose-primed AFM cantilevers with cells expressing rbSGLT1 (G6D3). (A) The sodium dependence of binding, (B) the most probable unbinding force fu and (C) the inhibition of binding by phlorizin; binding of cells not expressing rbSGLT1 (CHO) is shown as a comparison.25 |
The specificity of interaction could also be confirmed by blocking the sugar binding site with phlorizin (Fig. 8C). These data establish that the binding events recorded occur at the surface of SGLT1 molecules. The vinyl sulfone–PEG800–NHS cross-linker was purposely selected for this investigation since the bulky vinyl sulfone group present at the end of the linker most probably prevents a translocation, and therefore, only initial D-glucose binding events to SGLT1 should be observed. It is proposed that substrate transport by SGLT1 proceeds in several steps along the translocation pathway involving conformational alterations of the carrier.31,37,41,42 Our results demonstrate directly that the sugar binding site is accessible only when sodium is bound to the carrier, which opens the outward-facing gate of the transporter.7
When the effect of various sugars on the binding probability of the 1-thio-D-glucose tip to the transporter was investigated, a stereo-selectivity differing from that obtained in transport studies was found.23 The results suggest an initial binding site, which represents a first selectivity filter and selects sugars with regard to D- or L-conformation and the presence or positioning of OH groups at C1, C3, C4, and C6 but not at C2. The rejection of 2-deoxy-D-glucose, which is not transported, has to occur later during a subsequent binding/transport step. A similar discrepancy between initial binding and translocation has been observed previously in the rat kidney proximal tubule. 2-Deoxy-D-glucose was shown to inhibit binding of phlorizin to isolated brush border membrane vesicles but not transepithelial transport in microperfusion studies.43,44 Thus, the stereospecificity of transport is determined by at least two different selectivity filters, one located at the surface of the transporter, probably in or formed by the vestibule, and the other close to Gln457 and Thr406 in the translocation pathway.
Furthermore, an antibody against subdomain II partly inhibits the interaction of glucose with the transporter. Conversely, glucose inhibits the interaction of an antibody with subdomain II (see Fig. 9).
Fig. 9 Conformational changes in subdomain II in the presence of D-glucose in SGLT1-expressing cells. Distance–force cycles were performed with the cantilever primed with an antibody against subdomain II. (A) The reduction in binding of the antibody in the presence of D-glucose and when the binding sites are saturated with free antibody in solution. In the absence of sodium, no significant effect of D-glucose was observed (B). Asterisks indicate statistical significance, for further details see ref. 23. |
These findings also support the idea that the three subdomains form a vestibule containing the initial outside-facing interaction sites of the transporter and undergo significant conformational changes during the binding process.
Fig. 10 Interaction of a phlorizin-primed AFM cantilever with right-side-out oriented brush border membrane vesicles isolated from the rat renal cortex. The upper panel shows reduced binding in the presence of free phlorizin (Pz), and the lower panel shows inhibition of binding by high concentrations of D-glucose.46 |
Experiments were also performed using an AFM cantilever tethered with an antibody directed against the epitope aa 603–630 of subdomain III. In the presence of phlorizin, the probability of antibody binding was drastically reduced, confirming a strong change in conformation of this ectodomain induced by phlorizin binding. Specific binding of an AFM cantilever primed with phlorizin to SGLT was also detected in SGLT 1 expressing cells.12 In addition, the changes in conformation of subdomain III after phlorizin binding were confirmed in intact cells.12
The decrease in the average lifetime for phlorizin suggests that the aglucone binding sites for transport inhibitors have specific, temperature-sensitive conformations. These conformations will be investigated in the next sections.
Fig. 11 Modeling of interactions of subdomain III with phlorizin. The regions between TMH 12 and 13 of the vSGLT transporter structure (PDB ID: http://www.rcsb.org/pdb/explore.do?structureId=3DH4) were selected as templates for helices H1 and H2 (in green) as described in detail in ref. 48. Phlorizin (Pz) is shown in gray. (A, front view) The 4-OH of ring B of phlorizin is shown to interact with Arg-602 in H1, the 6-OH of ring B with residues 606–609 and the 4-OH of ring A with/around Asp-611. (B, side view) The glucose moiety of phlorizin is highlighted which is pointing towards the sugar binding domain depicted in green. Interactions between the OH groups of glucoside and several amino acids in the sugar binding domain of SGLT1 are also depicted. Modeling was performed using a PyMol computer modeling program (http://www.pymol.org/).48 |
Fig. 12 Modeling of the interactions between hexyl-glucoside and subdomain III. The data were obtained in studies with tryptophan mutants of isolated subdomain III in solution.47 The modeling of the interactions of hexyl-glucoside with regions between TMH 12 and 13 of the vSGLT transporter structure (PDB ID: http://www.rcsb.org/pdb/explore.do?structureId=3DH4) was performed using a PyMol program as described in Fig. 11. The interaction of C2 of the alkyl chain of HG with the region around residues 598–600 of helix 1 and C6/C8 of the alkyl chain with the region between residues 624 and 630 in helix 2 is depicted. Similar to the phlorizin–subdomain III complex, the glucose moiety is free to interact with the sugar binding domain depicted in green. The red arrows indicate flexibility of the alkyl side chain for proper interaction in the binding. |
When both models (phlorizin and hexyl-glucoside models) are compared, the glucoside moiety of phlorizin is slightly above the plane of that of the hexyl-glucoside, agreeing well with the idea that aglucone binding domains are flexible to move with regard to the membrane plane.
If phlorizin or alkyl-glucosides interact with the accessible extramembranous part of loop 13 (subdomain III), they first interact via their aglucone moiety while pushing the aglucone–loop 13 complex into the membrane to interact with the sugar translocation pathway. These changes in conformation of subdomain III are in agreement with the inhibitory effect of phlorizin on the interaction of a cantilever primed with an antibody against subdomain III (see above). Thus, after phlorizin binding to the transporter, the epitope (aa 606–630) is no longer accessible to the antibody PAN3-2. This change could be due to an obstruction of the antibody binding sites by phlorizin itself or due to a conformational change in the transporter. Support for the former assumption is rather weak because the epitope is much larger than the region between amino acids 602 and 611, which, as detailed above, acts as a phlorizin-binding domain.35,46,47,49 Since it has been shown that endodomains of the C-terminal part (region between transmembrane helices 10–13) are responsible for sugar translocation, we rather assume that phlorizin induces a movement of subdomain III which brings it close to or even into the plasma membrane plane, thereby making the interaction with sugars and thus their translocation impossible.
Fig. 13 Schematic representation of phlorizin interaction with subdomain III of various members of the SGLT family. Qualitatively similar folding patterns of phlorizin binding domains are predicted for SGLT1–4, except for vSGLT, which lacks secondary structure contents and does not exhibit a proper phlorizin binding pocket. The ranking of phlorizin interaction is depicted based on previously described phlorizin inhibition studies and our prediction analyses. The gradient filled arrow (in gray) represents the magnitude of phlorizin interaction/inhibition in various SGLTs.48 |
Furthermore, we found a strong correlation between the length of the C-terminus and phlorizin inhibition. The weakest phlorizin inhibition in vSGLT is probably caused by the absence of a long C-terminus as well as a proper phlorizin binding domain. However, SGLT1–4 carry an extended C-terminus/loop 13 as well as secondary structures in phlorizin binding domains, thereby exhibiting higher sensitivity. These predictions strongly agree with the previously reported phlorizin inhibition kinetics with the following ranking: SGLT2 > SGLT1 > SGLT4 > SGLT3 ≫ vSGLT. Interestingly, the sugar binding residues were also found to be quite conserved among these SGLT members, thereby indicating a common mechanism by which other SGLTs are inhibited by phlorizin or its high affinity analogs.48
Structurally similar analogs of phlorizin, like dapagliflozin and canagliflozin, exhibit better absorption in the gastrointestinal tract than phlorizin. Considering that these analogs share the same binding pocket as phlorizin,50 our predictions are very useful in understanding the mechanism of SGLT inhibition. Based on primary sequence analyses and computer modeling prediction, the increase in secondary structural contents (helices H1, H2 and H3) could promote high specificity and strong affinities of phlorizin and its analogs for SGLT2 as compared to SGLT1.48 These assumptions fit quite nicely with the recently illustrated homology modeling and molecular dynamics simulation studies predicting higher stability of SGLT2 binding complexes than SGLT1, and an increase in hydrophobicity might also promote hydrogen bonding within the binding pocket upon inhibitor binding.27 Furthermore, for SGLT2 an additional binding of the B ring of phlorizin to H3 is expected which could explain the high affinity of dapagliflozin, which has an extended CH2–CH3 chain at C6 of the B ring.
SLC | Literature name | Function | Drug/inhibitor | Potential ectodomain | Remarks | Ref. |
---|---|---|---|---|---|---|
SLC2 | GLUT1 (SLC2A1) | Glucose transport | Phloretin | Extracellular vestibule (infundibulum) | There is an additional intracellular binding site at the exit of the transport channel | 5, 51 |
Forskolin | ||||||
SLC6 | SERT (SLC6A4) | Na/Cl/monoamine cotransport | Tricyclic anti-depressants (TCA) | Extracellular vestibule | Transient, low affinity, noncompetitive interaction | 26, 52, 53 |
DAT (SLC6A3) | Serotonin | High affinity binding in the substrate binding site | ||||
NET (SLC6A2) | Dopamine | |||||
Noradrenalin | ||||||
SLC12 | NKCC1 (SLC12A1) | Na/K/2Cl cotransport | Loop diuretics: furosemide, bumetanide | Extracellular part of a transmembrane helix | Bumetanide: transient interaction at the extracellular entry point of TMH 3, high affinity binding at the inner end of TMH 3 at a chloride binding site. Furosemide: less affected by mutations suggesting additional binding sites | 2, 54 |
SLC5 | SGLT (SLC5A1, SLC5A2) | Na/glucose cotransport | Phlorizin | Extracellular vestibule | The sugar moiety of the beta-glucoside phlorizin binds in addition to the sugar translocation site | This review |
Phloretin |
Thus, in the sodium-independent glucose transporter, GLUT1, phloretin is found in homology building, molecular modeling and docking studies both in the extracellular vestibule and at the intracellular exit of the transport channel. The same holds for forskolin, whereas cytochalasin B acts only at an intracellular site.51 In the monoamine transporter, there is some evidence that a weak transient interaction of tricyclic antidepressants in the extracellular vestibule is followed by strong binding to the substrate binding site which is of competitive nature.26,52,53 For the sodium–potassium–chloride cotransporter, a transient interaction at the entry point of a transmembrane segment that is part of the ion translocation pathway might precede the competitive binding to a chloride binding site deep in the protein. Furosemide appears to have additional interactions with the transporter. It should be pointed out that in most of the studies mentioned above modeling and simulations are the basis of the conclusions and thus require further investigations such as crystallization of the complexes; direct experimental evidence for ectodomain–inhibitor binding has only been provided for SGLT1.
Thus, we would propose a common mechanism (including SGLT1) for inhibition. Recognition events take place at the ectodomain level, and then, the inhibitors travel through vestibules via multiple binding sites and finally bind strongly in the cavity of the transporter. In this regard, the crystal structure of SLC6 in the presence of an inhibitor55 nicely complements our functional/modelling studies and agrees well with the idea that inhibitors of the SLC family are recognized in the ectodomain regions before the second high affinity binding event takes place in the transmembrane region, e.g. phlorizin binding to loop 13 (ectodomain level) and its glucoside binding within the sugar binding pocket (transmembrane region), by repositioning of various parts of the transporter and the inhibitor during inhibition.
The studies presented above clearly indicate that ectodomains of the transporter molecule can have quite stable substructures which can provide selective binding sites for additional chemical entities of the inhibitors, not interacting with the substrate binding pockets. They, therefore, have to be included in modelling transport inhibitor complexes, docking experiments or virtual screening techniques.56
Functional roles of ectodomains have been described for a variety of transporters57–59 which point to additional potential target–inhibitor interaction sites. Another reason to take ectodomains close to the substrate binding pocket into account is that, in contrast to the high homology/similarity in the amino acid sequence of transport translocation pathways, ectodomains differ considerably amongst members of a transporter family, as could be demonstrated for the SGLT family in this review. This opens the possibility that different members of the transporter family, which are usually expressed in different organs, might be targeted by modification of the ectodomain binding entities of the drug. In more general terms, selectivity probably can be improved by targeting secondary binding pockets with extended ligands.
Footnotes |
† The authors declare no competing interests. |
‡ Contributed equally. |
This journal is © The Royal Society of Chemistry 2016 |