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Copyright © 2007 The Biophysical Society. All rights reserved.
Biophysical Journal, Volume 92, Issue 2, L23-L25, 15 January 2007

doi:10.1529/biophysj.106.097311

Biophysical Letters

Membrane Simulations of OpcA: Gating in the Loops?

Peter J. Bond^*, Jeremy P. Derrick^† and Mark S.P. Sansom^*, ,  

^* Department of Biochemistry, University of Oxford, Oxford, United Kingdom
^† Faculty of Life Sciences, University of Manchester, Manchester, United Kingdom

Address reprint requests and inquiries to Mark S. P. Sansom, Tel.: 44-1865-275371; Fax: 44-1865-275273.

Progress in structural biology has yielded ∼110 distinct high resolution membrane protein structures. However, it appears that the experimental conditions under which a membrane protein structure is obtained, e.g., presence of detergent/lipid 1, crystallization solutes 2, or pH 3, may influence aspects of its conformation. This is important when trying to relate (static) structure to (dynamic) biological function. Molecular dynamics (MD) simulations yield dynamic information on membranes 4. MD is used here to investigate loop mobility in relation to ligand binding and the possibility of channel gating in the outer membrane protein (OMP) OpcA. OpcA is an adhesion protein from Neisseria meningitidis implicated in the development of meningitis and septicemia in humans. OpcA is thought to mediate attachment to host cells by binding proteoglycan cell-surface receptors. Its x-ray structure 5 shows that OpcA forms a 10-stranded β-barrel, with five highly mobile extracellular loops. The loops form a positively charged crevice that could theoretically accommodate proteoglycan. However, fluorescence-based binding studies suggest the binding site may be in a different location, near to a tyrosine residue (Tyr-169) adjacent to residues in loop L2 6. Moreover, whereas the β-barrel interior of OpcA is water-filled and rather wide (mean radius ∼0.2nm), loop L2 adopts an unusual conformation, traversing the barrel axis and thereby preventing formation of a continuous pore.

Thus, the conformation of the loops is important in understanding both the mechanism of host cell adhesion and the possibility of pore formation by OpcA. Zn²⁺ ions were necessary for formation of OpcA crystals. Crystallographic densities for three such ions were identified in the structure, one within the central cavity in the interior of the β-barrel and two on the extracellular surface in the loops that mediate crystal packing interactions. It is therefore of interest to establish how more “physiological” conditions might alter the conformation of the protein. Thus, two 20ns MD simulations were carried out for OpcA in a lipid (dimyristoyl-phosphatidylcholine) bilayer, in either ∼0.1M or ∼1M NaCl (Fig. 1). (Details in Supplementary Material .)

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Figure 1

Snapshot of OpcA (cutaway blue cartoon format) within a dimyristoyl-phosphatidylcholine bilayer (light blue) surrounded by water (red/white), with ions omitted for clarity.

The C^α root mean-squared deviation (RMSD) allows the measurement of the drift of the protein from its initial crystal-derived conformation (Fig. 2). In both simulations, the β-barrel domain of OpcA proved to be particularly stable, with the RMSD peaking at to 0.15–0.2nm within ∼5ns. In contrast, the extracellular loops showed much greater conformational drift, with an RMSD of ∼0.4nm within the first ∼5ns, and final values reaching 0.4–0.45nm by 20ns. Consistent with its length and lack of defined structure, loop L2 seemed to be the primary contributor to this high RMSD, with localized sections exhibiting large twisting motions, as indicated by principal component analysis.

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Figure 2

Cα RMSD in the 0.1M (thick lines) and 1M (thin lines) simulations for the barrel and extracellular loops.

The large RMSD in the extracellular loops appears to be a result of the absence of Zn²⁺ ions and crystal-packing contacts. Specifically, the side chains of residues Asp-69, His-128, and Thr-176 (in loops L2, L3, and L4, respectively) and Glu-223 (in loop L5 of an adjacent monomer) were within 0.35nm of one Zn²⁺ ion. Moreover, a salt-bridge is present between the L5 loops of adjacent monomers. Visual inspection of the simulations indicated significant conformational changes in these loop regions. Two small α-helices in loops L2 and L4 completely (0.1M simulation) or partly (1M simulation) unfolded (Fig. 3), whereas a small β-strand section in L2 formed in the 0.1M system. Moreover, these changes were propagated to loop L5, where a small β-hairpin grew by a few residues. The higher ion concentration seems in part to stabilize the crystallographic-induced loop structure in comparison with the 0.1M simulation. This was confirmed by calculating the simulated C^α B-factors, which showed consistently higher loop fluctuations for the 0.1M simulation. Although the highest region of mobility in the protein for each simulation was observed in loop L2, each peaking around Gly-74, which lies at the tip of the loop, the relative magnitude is significantly greater for the 0.1M simulation (∼300Ų) than the 1M simulation (∼50Ų). The difference may arise from a greater extent of ionic interactions with charged residues in the loops of OpcA (L2 alone contains six Lys residues and four Asp/Glu residues).

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Figure 3

Snapshots of the extracellular surface of OpcA (gray cartoon format) for the crystal structure (left) and at 20ns for the 0.1M MD simulation (right). In the crystal, a crevice (black arrow) is formed primarily between loop L2 (red cartoon format surrounded by its green molecular surface) and loops L1 and L5 (yellow molecular surface). Motions in loop L2 and L5 result in the closure of this cleft and the formation of a pathway (blue arrow) from the solvent to Tyr-169 (space-filling format).

Thus, it appears that whereas the Zn²⁺ ion and crystal contacts hold loops L2 and L4 together, they concurrently induce a possibly nonnative α-helical conformation. What impact might this have on our interpretation of the biological function of OpcA? In the simulations, the L1, L2, and L5 loop regions undergo significant changes in conformation, leading to changes in the crevice feature identified in the original OpcA structure. This site effectively closes off completely (in the 0.1M simulation) or partially (in the 1M simulation) (Fig. 3). On the other hand, in the crystal structure, two Pro residues (Pro-82 and Pro-86) in L2 lead to a tapering of the pore, due to a kink in the loop that covers the mouth of the barrel, before extending outward at a second kink (Fig. 4). It is noteworthy that residues Lys-80 to Thr-83 in loop L2 lie adjacent to Tyr-169 (Fig. 3), which plays a major role in the intrinsic fluorescence response to sialic acid binding 6. During simulation, the induced closure of the extracellular loop crevice is accompanied by the movement of L2 away from the barrel mouth and Tyr-169, supported by conformational changes in the tip of L1. Biologically, this may represent the first stage in the creation of a pathway required for binding proteoglycan receptors.

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Figure 4

Internal pore surface (green) (analyzed using HOLE 7) for the crystal structure (left) and open 0.1M simulation (right). Residues in L2 (red) and the barrel are indicated.

The two Pro residues in loop L2, along with the Glu-70/Lys-72 salt bridge at the tip of the loop (Fig. 4), result in the pore radius of OpcA being reduced to a minimum of ∼0.02nm at the mouth of a putative channel through OpcA. In contrast, the observed conformational changes in the loops during simulation result in a significant widening of the barrel mouth. In particular, at the main block to pore formation, at Pro-82, the radius in both simulations is increased to ∼0.1nm on average over the final 15ns, and the large fluctuations in pore radius along the whole length of loop L2 mean that the entire barrel mouth is significantly opened in comparison with the crystal structure. Consequently, a continuous pore can be found along the length of the protein for long periods of each simulation (Fig. 4). This is formed beyond the Arg-109/Lys-252 pair at the intracellular mouth, through the His-13/Arg-39/Arg-51 triad, and out of the now widened extracellular mouth, past the pair of Pro residues and through the center of L2.

It should be noted that no ions were observed to pass through the pore in either simulation, as the simulation time is likely to be an order of magnitude lower than the time required for the diffusion of a single ion through a transmembrane pore. Nevertheless, multiple water molecules were observed to traverse the length of the pore, bypassing the pair of Pro residues that originally blocked the barrel mouth in the crystal structure. For comparison, a short (7ns) simulation was performed, in which the loop residues involved in coordinating the Zn²⁺ ion were restrained relative to one another. Despite these restraints, significant changes in the surrounding loop regions were observed (see Supplementary Material ), enabling a few water molecules to pass through the pore. This suggests that the crystal contacts between loops of adjacent OpcA monomers help to maintain the conformation of loop L2.

It should be noted that OpcA has not been reported to form ion permeable pores. However, assuming that OpcA is filled with a 1M KCl solution, based on the simulated pore size, the conductance of a putative OpcA channel was predicted to be ∼100 pS 7. Interestingly, the minimum pore radius fluctuates significantly on a nanosecond timescale due to the Pro kinks in loop L2, leading to variation in predicted conductance over each simulation of between ∼0 and 250ps. Similar flickering patterns of conductance have also been observed via simulated 8 and experimental 9 measurements for OmpA.

The simulation study presented here reveals that the absence of crystal-packed neighboring proteins and Zn²⁺ ions, and the presence of a more biologically relevant bilayer, result in concerted conformational changes in the extracellular loops. These loop motions result in the unblocking of the pore toward the extracellular mouth of the β-barrel, as well as rearrangement of external surface of OpcA. The simulations indicate that the ligand binding site may be quite dynamic, suggesting the possibility of an induced fit mechanism. The movement of loop L2 away from Tyr-169 is supportive of a mechanism in vivo whereby conformational changes in the extracellular loops precede proteoglycan binding. Interestingly, raising the salt concentration in our simulations resulted in higher protein stability and a consequent moderation of these effects. This is pertinent in the light of recent crystal structures of a 14-stranded β-barrel protein, OmpG 3. The study revealed that the pH gated opening of its pore is effected via structural changes in a long extracellular loop, which is folded across the barrel in the closed state only. Moreover, Gd³⁺ ions have been shown to close OmpG 10, whereas Ca²⁺ ions were observed to bind to the extracellular loops. Similarly, in plant aquaporins, a loop blocks the channel from the cytoplasm but upon displacement opens the pore 11. Binding of divalent cations near this gating loop has been implicated in regulation. It therefore seems feasible that sensing the local environment via structural changes in extracellular loops may be a common theme for membrane proteins. In the case of OpcA, this may affect ligand binding, thereby aiding the correct identification of specific host sites for successful adhesion of N. meningitidis cells, the first step in the pathogenesis of disease. This is especially important as OpcA needs to recognize the sialic acid on the surface of epithelial cells while surrounded by a “sea” of lipopolysaccharide rich in sialic acid in the bacterium’s own outer membrane surface. It will therefore be of interest to extend simulations of OpcA and other outer membrane proteins to a model of the environment provided by the lipopolysaccharide of Gram-negative bacterial outer membranes 12.