Volume 2012 (2012), Article ID 520307, 7 pages
Hydration Water Freezing in Single Supported Lipid Bilayers
1Department of Physics & Astronomy, McMaster University, 1280 Main Street West, Hamilton, ON, L8S 4M1, Canada
2NIST Center for Neutron Research, NIST, Gaithersburg, MD 20899, USA
3Department of Materials Science and Engineering, University of Maryland, College Park, MD 20742, USA
4Canadian Neutron Beam Centre, National Research Council Canada, Chalk River, ON, K0J 1J0, Canada
Received 2 January 2012; Accepted 31 January 2012
Academic Editors: J. P. Bradshaw, L. Loura, and J. Perez-Gil
Copyright © 2012 Laura Toppozini et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
We present a high-temperature and high-energy resolution neutron scattering investigation of hydration water freezing in single supported lipid bilayers. Single supported lipid bilayers provide a well-defined biological interface to study hydration water dynamics and coupling to membrane degrees of freedom. Nanosecond molecular motions of membrane and hydration water were studied in the temperature range 240 K < T < 290 K in slow heating and cooling cycles using coherent and incoherent elastic neutron scattering on a backscattering spectrometer. Several freezing and melting transitions were observed. From the length scale dependence of the elastic scattering, these transitions could be assigned to freezing and melting of hydration water dynamics, diffusive lipid, and lipid acyl-tail dynamics. Coupling was investigated by comparing the different freezing and melting temperatures. While it is often speculated that membrane and hydration water dynamics are strongly coupled, we find that membrane and hydration water dynamics are at least partially decoupled in single bilayers.
Despite the vast potential for applications of single membranes in biotechnology and fundamental research [1, 2], experiments using single membranes are challenging, mainly because of the small amounts of sample material and corresponding small sample signals. Recent developments in neutron scattering instrumentation, and the increasingly powerful neutron sources, have made it possible to experimentally address molecular dynamics in single bilayers. Lipid diffusion in single supported bilayers made of DMPC (1,2-dimyristoyl-sn-glycero-3-phosphatidylcholine) was studied recently using quasielastic neutron scattering . A freezing transition at T = 271 K was reported and associated with freezing of hydration water molecules. Here, we used solid-supported single-lipid bilayers as a well-defined biological interface to study freezing and melting of hydration water and membrane.
We report a high-energy and temperature-resolution neutron scattering study using a backscattering spectrometer in a temperature range between 240 K and 290 K. While the temperature range 100 K < T < 220 K was investigated thoroughly in the literature to study the so-called “dynamical transition” in hydrated protein and membrane systems, much less attention was paid to the onset of freezing at 271 K in the past. By analyzing the length scale dependence of the elastic coherent and incoherent scattering, freezing of hydration water and membrane dynamics was observed, and the corresponding freezing and melting temperatures determined. Single supported bilayers of the model membrane system DMPC were prepared on silicon wafers, as shown in Figure 1. Diffusion of lipid molecules, lipid acyl-tail dynamics, and dynamics of hydration water molecules were studied simultaneously using protonated lipids, hydrated by heavy water (D2O). We measured nanosecond molecular dynamics on the High Flux Backscattering Spectrometer (HFBS) at the NIST Center for Neutron Research, Gaithersburg, via elastic neutron scattering experiments. Fixed energy-window scans (FEW-scans) centered at zero energy transfer were recorded as a function of sample temperature to probe molecular motions on a time scale as long as ~1 ns. A freezing transition at T = 271 K was observed upon slow cooling of the sample. This transition has previously been observed not only in single supported  but also in stacked membrane systems [7–10] and was assigned to freezing of membrane hydration water. We find evidence for additional freezing and melting transitions that we assign to hydration water molecules and membrane dynamical degrees of freedom. Coupling between hydration water, lipid diffusion, and lipid acyl-tail dynamics was studied by comparing the corresponding freezing and melting temperatures.
2. Materials and Methods
2.1. Sample Preparation
Single supported bilayers of the model system DMPC supported on silicon wafers were prepared by vesicle fusion [11–13] using the protocol reported in : Double-side polished, 2′′ Si(100)—wafers were cleaned by immersing the wafers in an H2O2 + sulfuric acid mixture (volume fraction of 70% concentrated H2SO4, 30% H2O2 at 90°C for 30 min). This strongly oxidizing combination removes all organic contaminants on the surface but does not disturb the native silicon oxide layer. The wafers were then rinsed and stored under distilled water before use . 200 mL of a mol/L Hepes, mol/L MgCl2, and mol/L KCl buffer solution was prepared and heated to 55°C. 1,2-dimyristoyl-sn-glycero-3-phosphatidylcholine (DMPC) was added to the buffer solution up to a concentration of 1.5 mg/mL. The milky suspension, which initially contained multilamellar lipid suspensions, was sonicated (50% duty cycle, power level 4) for 15 h until the suspension became transparent and small unilamellar vesicles formed. The hydrophilic Si wafers were then completely immersed in the suspension for 1 hour. The lipid suspension was kept at 55°C during the whole process to keep the bilayers in their fluid phase. After 1 h, the wafers were thoroughly rinsed with ~2 L of ultra pure water to remove excess vesicles from the surface. By applying this procedure, small bilayer patches initially develop on the substrate, which eventually undergo a transition into a large uniform single bilayer after approximately 20–25 min . The substrates were then annealed for 72 h at 55°C in an oven in air before mounting in an aluminum sample can, and rehydrated. To check the existence of a a single supported bilayer, the quality of the samples was checked by atomic force microscopy (AFM) and X-ray reflectivity. AFM pictures showed a defect-free uniformly covered surface. From the absence of sharp Bragg peaks in the X-ray experiment, a multilamellar structure could be excluded.
To increase the scattering signal, 100 double-sided, polished wafers (resulting in 200 single bilayers) were mounted horizontally into the neutron spectrometer, with the plane of the bilayers in the scattering plane, as depicted in Figure 1. The sample was sealed in an aluminum sample can and placed inside a closed-cycle refrigerator (CCR) during the experiment. The experimental temperature range extended from of 240 K to 290 K, where freezing of the hydration water molecules was expected. 120 μL of heavy water was added before closing to ensure full hydration of the bilayers. The sample can used in this study was designed such that the formation of bulk ice is discouraged in the experimental setup, such as on the windows of the sample can or on the sample, and would occur outside of the neutron beam.
2.2. Neutron Scattering Experiment
The neutron experiment was carried out at the high flux neutron backscattering spectrometer HFBS at the NIST Center for Neutron Research (NCNR), Gaithersburg,  in its standard setup with Si(111) monochromator and analyzer crystals corresponding to an incident and analyzed neutron energy of 2.08 meV ( = 6.27 Å). At the resolution of 0.8 eV, only molecular motions with characteristic times slower than 1 ns are monitored. The experiment covered lateral length scales of 3.5 Å to 12 Å to study in-plane dynamics down to nearest neighbor distances of lipid acyl tails and hydration water molecules. Performing so-called “elastic’’ scans, which record the elastic scattering intensity as a function of temperature, reveals dynamical changes on different length scales. Freezing and melting of molecular degrees of freedom can easily be identified because they lead to jumps or kinks in the recorded intensity. The counting time per scan was 5 minutes. Using cooling and heating ramps of 0.04 K/min, this results in a temperature resolution of 0.2 K. The 16 HFBS detectors (D1–D16) cover a total Q range of 0.14 Å−1 to 1.81 Å−1. The Table 1 lists the center Q values and the corresponding length scales. Each analyzers covers an angular range of approximately 8deg. As the membranes were oriented with the membrane plane in the scattering plane, the observed Q values were all oriented in the plane of the membranes, .
Different types of motion fall into the length scales covered by the HFBS spectrometer. Atomic and molecular motions in membranes can be classified as local, self-correlated, and collective, pair-correlated dynamics. Local dynamics correspond to the motion of molecules or functional groups in local energy potentials. The force and time constants involved are determined by the local friction and restoring forces. This type of dynamics is called incoherent because the particles move independently in their local environments. Examples are vibration, rotation, libration (hindered rotation), and diffusion of individual lipid molecules. Coupled, collective molecular motions arise due to an interaction between particles or functional groups. This type of dynamics is called coherent. Collective molecular motions determine, for instance, elasticity of membranes  and interactions between membrane embedded proteins , and are important for membrane transport [19, 20]. Within the scattering formalism, incoherent, autocorrelated dynamics is described by the incoherent scattering function, , while the coherent scattering, , describes dynamics involving different molecules [21, 22].
Different types of dynamics can be distinguished based on their length scale dependence: Gaspar et al. have recently shown that incoherent and coherent scattering contributions in proteins can be discriminated by using neutron polarization analysis . By using protein powders at different levels of hydration, scattering contributions due to the hydration water could be identified: The nearest neighbor distance of the hydration water molecules leads to a correlation peak centered at 1.85 Å−1, corresponding to a distance of 3.4 Å between hydration water molecules. Detector D16 was, therefore, assigned to dynamics of hydration water molecules.
The lipid acyl chain correlation peak in DMPC is the result of a close packing of the lipid tails in the hydrophobic membrane core. The corresponding correlation peak occurs at ~1.5 Å−1 in the gel phase [10, 19] (below the main phase transition at T = 294 K), corresponding to a nearest neighbor distance of 4.2 Å. Detector D13, which covers this length scale, was, therefore, assigned to lipid tail dynamics. Lipid and water dynamics were studied previously using backscattering spectrometers by analyzing elastic scattering at the positions of the lipid acyl chain and hydration water correlation peaks [9, 10, 23]. These studies demonstrated that the different length scales and corresponding detectors are decoupled and that lipid and water dynamics can be studied separately but simultaneously.
Incoherent scattering is dominant at intermediate values, between 0.3 and 1.5 Å−1, where no correlation peak occurs. This range of length scales between ~4 and 21 Å is often used in neutron scattering studies (see, e.g., [7, 8]) to study diffusion and molecular mean square displacements of lipid molecules. We assigned the Q range from 0.6 Å−1 to 1.05 Å−1 (detectors D5–D8), covering length scales from 6.3 Å–10 Å to incoherent dynamics due to diffusion of lipid molecules.
Lipid diffusion and lipid and hydration water dynamics were studied simultaneously by analyzing different detectors. Table 1 lists the dominant scattering contribution for the different length scales, and the corresponding type of motion observed in the various detectors. The HFBS analyzers cover an angular range of approximately 8° each. The experiment was, therefore, not sensitive to shifts of the lipid and water correlation peak with temperature within this resolution due to potential structural changes of the bilayers with temperature.
Data were collected during cooling and heating cycles, using a temperature ramp of 0.04 K/min. The temperature ramp of 0.04 K/min was determined to be in thermal equilibrium as there were no observed differences to data taken at even slower speeds. Note that faster ramps could lead to partial dehydration of the membranes because of a possible temperature gradient inside of the sample can.
Figure 2 depicts the elastic scattering collected from detectors D5–D8, D13, and D16, which represent lipid diffusion, (a), lipid tail dynamics, (b), and hydration water dynamics, (c). The elastic scattering due to lipid diffusion increases upon cooling until a freezing transition is observed at T = 264 K (3). A second step occurs at T = 252 K (5). The membrane shows a hysteresis in the heating curve, which was shifted upward on the intensity axis for clarity. During the heating cycle, the melting transition is observed to begin at T = 271 K (2). The membranes transition back into their high temperature state at 279 K (1).
Lipid tail dynamics were studied in detector D13, which collects scattering at the position of the lipid acyl chain correlation peak. The freezing curve in Figure 2(b) shows two pronounced anomalies corresponding to freezing transitions, the first at T = 264 K (3), and the second at T = 255 K (4). The temperature of transition (3) in D13 agrees with the transition observed in detectors D5–D8. The heating curve (shifted upward on the intensity axis for clarity) shows transitions at T = 247 K (6), T = 252 K (5), T = 271 K (2) and T = 279 K (1).
Hydration water dynamics were observed in detector D16 in Figure 2(c). The elastic intensity in Figure 2(c) shows a first kink at T = 271 K (2) in cooling. A second freezing transition is observed at T = 252 K (5). Two kinks corresponding to melting transitions can be assigned to the heating curve, at 252 K and 271 K. We note that the hydration water correlation peak occurs at =1.85 [9, 10, 15]. D16 does, therefore, not cover the entire water correlation peak. We argue, however, that D16 covers part of the broad hydration water peak (see ) to capture hydration water dynamics. All transition temperatures are listed in Table 2.
An empty aluminum can consisting of silicon wafers (without membranes), and heavy water was measured as a reference. Scattering of the sample, was constant, and no freezing or melting transitions were observed in the temperature range .
The system was cycled several times through the temperature range . Note that the heating curves in Figure 2 have been shifted upward on the intensity axis to distinctly show the transition locations. The original data shows closed loops for all plots, and the system always returned to its initial high-temperature state. The number of particles in the beam was constant, as the intensities of the elastic scattering at the beginning and end of the temperature cycle coincide, resulting in perfectly reproducible data. The cooling and heating rate of 0.04 K/min was slow enough such that the observed states were thermodynamic states rather than determined by hydration kinetics. The absence of a freezing transition at T = 277 K, the freezing and melting transition of heavy water, in Figures 2(a), 2(b), and 2(c) excludes the presence of bulk D2O in the beam. The dynamical changes in Figure 2 were, therefore, attributed to dynamical changes of the hydrophobic membrane core and the hydration water molecules.
The onset of freezing at transition (2) in the hydration water scan in Figure 2(c) can be compared to freezing of membrane hydration water in stacked membrane systems as reported from neutron diffraction  and elastic neutron scattering experiments [8–10]. The transition temperature of 271 K agrees well with the temperatures reported. Freezing of these hydration water molecules is supercooled by 6 K as freezing and melting of bulk D2O occurs at 277 K. A second freezing transition was observed at lower temperatures of T = 252 K.
Lipid diffusion and the lipid tail dynamics start to freeze at T = 264 K (3). The onset of freezing of membrane dynamical degrees of freedom appears to be decoupled from the hydration water freezing. Lipid diffusion shows a second freezing transition at 252 K, which coincides with the low-temperature hydration water freezing transition. Freezing of the hydration water molecules seems to have a strong effect on the displacement of lipid molecules. Lipid tail dynamics, however, appear to be less sensitive to hydration water dynamics, as the low temperature freezing in Figure 2(b) occurs at T = 255 K, slightly higher than the water freezing. Freezing transitions at ~250 K were also observed in the elastic neutron scattering and computer simulation data by Wood et al.  obtained in purple membrane. However, the relatively coarse temperature resolution in this study does not allow a quantitative comparison with the values in Table 2.
No hysteresis was found in freezing and melting of the hydration water; freezing and melting temperatures coincide in the scan in Figure 2(c). Hysteresis of 15 K and 19 K were observed for diffusive membrane and acyl-tail dynamics, as listed in Table 2. These values are significantly larger than the experimental temperature resolution, possible hysteresis of the experimental setup, and the maximum error in the determination of the transition temperatures and must, therefore, be attributed to the membrane.
Diffusive lipid and tail dynamics show a first melting transition at T = 271 K (2), the temperature of the first hydration water melting transition. Membrane dynamics fully melt and return to their high temperature state at (1), and diffusive and tail dynamics appear to be coupled in heating. The melting transition of lipid diffusion appears as a pronounced step in the data in Figure 2(a), while all other transitions manifest as kinks. An additional transition at T = 247 K in the tail dynamics is observed in the heating curve in Figure 2(b), which has no analogue in cooling. Taking into account a possible hysteresis, this points to further freezing transitions in the correlated tail dynamics at lower temperatures, outside the temperature window of this experiment.
As this is the first study of freezing and melting of hydration water and membrane dynamics in solid supported lipid bilayers, we can, at this point, not provide a full explanation and a detailed molecular model. In particular, computer simulations are needed to unambiguously identify hydration water molecules inside the lipid head group region and possibly assign the transitions observed to freezing of water molecules in different hydration shells and their coupling to membrane dynamics. We argue, however, that the two main conclusions of this work are robust: (1) the observation that diffusive and correlated lipid dynamics are to some extent decoupled and show different freezing temperatures, and (2) that hydration water and membrane freezing are at least to some extent de-coupled in single supported lipid bilayers and show different freezing and melting temperatures.
A comment is in order: while one leaflet of the bilayer is directly exposed to water molecules, the other is closely interacting with the silicon substrate, with only a few water molecules available to interact. This is likely to affect the motional freedom of the lipid head groups of the lower layer and their hydration water molecules. The technique presented in this paper is not capable of easily resolving signals from different leaflets. The observed freezing and melting transitions may, therefore, also be related to molecular freezing and melting in different leaflets. It is, for instance, well known that confinement can lead to a suppression or lowering of freezing transitions as a result of competing interactions with the confining surface.
Protein powders, proteins in suspension, or multilamellar membranes are often used as model systems to investigate the structure and dynamics of the hydration water, and its impact on membrane and protein dynamics [8, 24–28]. Here, we have for the first time used single phospholipid bilayers supported on a solid surface to study freezing and melting of membrane and hydration water. The upper leaflet of the bilayer, and with it the water adsorption sites in the lipid head group region, is in direct contact with saturated water vapor. By preparing such a well-defined biological interface, it will in future experiments be possible to obtain detailed information about structure and dynamics of the hydration water and its impact on membrane dynamics and dynamics of membrane-embedded proteins.
In summary, we studied freezing and melting of hydration water and membrane dynamics in single supported lipid bilayers using high energy resolution neutron scattering on a backscattering spectrometer. Membrane and hydration water dynamics were studied in the temperature range 240 K < T < 290 K in slow heating and cooling cycles. Several freezing and melting transitions were observed. From the length scale dependence of the elastic scattering, these transitions could be assigned to freezing and melting of the hydration water and freezing of lipid diffusion and lipid acyl-tail dynamics. The different dynamics appear to be partially decoupled in this single bilayer system as we observe different freezing and melting temperatures. The onset of hydration water freezing was found at T = 271 K. Freezing of lipid diffusion and lipid tail dynamics was observed at a slightly lower temperature of T = 264 K. Single-supported lipid bilayers present a well-defined biological interface to study hydration water dynamics and their coupling to membrane degrees of freedom. Because of its simplicity, this system should in particular be highly suited for computer simulations.
The authors thank the NIST Center for Neutron Research for the allocation of beam time. This paper utilized facilities supported in part by the National Science Foundation under Agreement no. DMR-0944772. This paper was partially funded by the Natural Sciences and Engineering Research Council of Canada (NSERC) and the National Research Council Canada (NRC).
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