Vitaliy
Oliynyk‡
a,
Christian
Mille‡
ab,
Jovice B. S.
Ng
a,
Christoph
von Ballmoos
c,
Robert W.
Corkery
bd and
Lennart
Bergström
*a
aDepartment of Materials and Environmental Chemistry, Stockholm University, 10691 Stockholm, Sweden. E-mail: lennart.bergstrom@mmk.su.se
bYKI, Institute for Surface Chemistry, 11486, Stockholm, Sweden
cDepartment of Biochemistry and Biophysics, Stockholm University, 10691 Stockholm, Sweden
dDepartment of Chemistry, Division of Physical Chemistry, KTH Royal Institute of Technology, Stockholm, Sweden
First published on 4th January 2013
We report a robust and versatile membrane protein based system for selective uptake and release of ions from nanoporous particles sealed with ion-tight lipid bilayers of various compositions that is driven by the addition of ATP or a chemical potential gradient. We have successfully incorporated both a passive ion channel-type peptide (gramicidin A) and a more complex primary sodium ion transporter (ATP synthase) into the supported lipid bilayers on solid nanoporous silica particles. Protein-mediated controlled release/uptake of sodium ions across the ion-tight lipid bilayer seal from or into the nanoporous silica carrier was imaged in real time using a confocal laser scanning microscope and the intensity changes were quantified. ATP-driven transport of sodium ions across the supported lipid bilayer against a chemical gradient was demonstrated. The possibility of designing durable carriers with tight lipid membranes, containing membrane proteins for selective ion uptake and release, offers new possibilities for functional studies of single or cascading membrane protein systems and could also be used as biomimetic microreactors for controlled synthesis of inorganic multicomponent materials.
Silicon dioxide has been shown to be a useful surface for fusion of liposomes and the subsequent formation of supported lipid bilayers.17 Between these substrates and the bilayer, several monolayers of water are located – making it a suitable environment for incorporated proteins that can freely diffuse in the membrane.18,19 Porous silica spheres are particularly attractive because of their endoskeleton-like structure, tunable internal pores and surfaces.20–24 Recent works have shown that nanoporous silica spheres can be coated with lipid bilayers25–28 and used as delivery vehicles into cells.29,30 A common approach to functionalize supported membranes with transmembrane proteins is to spread vesicles incorporating proteins (proteoliposomes) onto supports.
In a first step towards the construction of systems that can also control the uptake of specific ions, proton pumps have been incorporated into lipid bilayers supported onto porous silica spheres.23,30 Previous work showed that it was possible to form a supported lipid bilayer containing a transmembrane redox-driven proton pump, Cytochrome c Oxidase (CytcO), by fusion of small unilamellar vesicles with reconstituted CytcO onto the surface of colloidal nanoporous silica particles.30 It was demonstrated that the CytcO retains its functionality while the supported membrane system was shown to be proton tight, defining an interior particle compartment that is separated from the surrounding aqueous media. Further, studies have been performed where ATP synthase and bacteriorhodopsin were used in biomimetic scaffolds (sol–gel) and artificial organelles (polymersomes), functioning as support for proton transport coupled to the synthesis of ATP.29,30 Indeed, simple compartmentalized modules with partial cellular functions may also give us insight into early or minimal life forms (protocells).31
In this study, we go beyond proton transporters and demonstrate uptake and release of sodium ions across a supported membrane using gramicidin A and ATP synthase, a peptide and a multi-subunit transmembrane protein, respectively, which utilize different transport mechanisms. Gramicidin A is a dimer that assembles from two monomers of 15 amino acids each, and forms a cationic-selective channel of 4 Å that spans the lipid bilayer.32 Passive ion transport through the channel is driven by either an ion gradient or an electrical membrane potential. This peptide has been extensively used in biomembrane research due to its formation of stable channels in supported lipid bilayers that have different affinities for monovalent cations. Gramicidin A is used by soil bacteria as an antibiotic, killing gram-negative bacteria.33 Na+-dependent F1F0 ATP synthase, on the other hand, is a primary sodium ion transporter, that – when supplied with energy in the form of ATP – moves sodium ions across the membrane.34
Here, we report the successful incorporation of both gramicidin A and the more complex ATP synthase into lipid bilayers, deposited on synthetic, nanoporous silica spheres. For gramicidin A, the functional incorporation was confirmed by studying the passive transport of monovalent cations from the solution into the particle. In the case of ATP synthase, the addition of ATP drives the transport of ions across the membrane. The activity of both the passive and the active transport was followed in real time using dye loaded particles imaged using confocal laser scanning microscopy.
The ATP synthase was then reconstituted into SUVs. The SUVs were prepared by dissolving 20 mg soy PC in 2 ml liposome buffer (20 mM Tris–phosphate, pH 7, 5 mM MgCl2) followed by sonication for 3 × 30 s on ice using a tip-sonicator (MSE Soniprep 150, Labtec AG, Wohlen, Switzerland). Sodium cholate (1% final concentration) and purified ATP synthase in a lipid:
protein ratio 200
:
1 (w/w) were added to the suspension of SUVs. The protein/lipid solution was kept at 4 °C for 30 min followed by loading on a PD-10 gel filtration column (GE Healthcare), pre-equilibrated with liposome buffer. The final concentration of ATP synthase was approximately 0.3 ATP synthase/vesicle (i.e. two out of three liposomes are empty, not containing any enzyme).
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Fig. 1 Characterization of lipid bilayer coated nanoporous silica spheres. SEM images of the (a) monodisperse nanoporous silica (SNS) spheres and (b) their internal fractured surface that shows that the SNS is solid without a hollow core. (c) CLSM image of the SNS spheres sealed with DOTAP lipid bilayers containing 1–3% Texas Red® DHPE. (d) Intensity graph obtained along the white horizontal line representing the size of the particle. The CLSM images were obtained 7 days after sealing and subsequent storage at 5 °C. |
About 1–3% of Texas Red® DHPE lipid were mixed with the lipids to facilitate fluorescence imaging of the lipid coating. CLSM images obtained immediately after coating (not shown) and after 7 days of storage at +5 °C (Fig. 1c and d) show that the supported lipid bilayers (red rings) exhibit long-term stability. The relatively small pore size of the SNS used in this study is well below the critical pore size of 10 nm that was shown by Davis et al.23 to be the upper limit for the formation of stable lipid bilayers onto the outer surface of mesoporous silica particles. The durability and permeability of the supported-DOTAP or -DLPC lipid bilayers were evaluated by following the diffusion of fluorescent dyes that were preloaded into the SNS particles prior to lipid bilayer sealing.
Fig. 2 shows that the intensity of fluorescein inside the lipid bilayer-sealed particles remains virtually unchanged while the intensity of the uncoated SNS drops dramatically over time. This observed drop in fluorescence intensity is consistent with the results obtained in a previous study where small negatively charged dye molecules were released from uncoated mesoporous spheres within 5–7 hours.36 Similar experiments on negatively charged Oregon Green and positively charged Rhodamine 6G show that DOTAP and DLPC supported lipid bilayers are able to effectively seal the molecules inside the porous carriers.
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Fig. 2 Time evolution of the release of fluorescein from; (a) SNS particles sealed with DLPC lipid bilayers; (b) unsealed SNS. |
Fig. 3b shows a CLSM image of the membrane protein-containing lipid bilayer coated porous particles where the SG-loaded interior sphere (green) and the Texas Red-labeled lipid bilayers coating (red ring) are clearly distinguished. The CLSM images in c show that SNS particles sealed with DLPC lipid bilayers, containing 1 mol% of gramicidin A, are only weakly fluorescent (low quantum yield). Exchange of the external media from 100 mM KCl to 100 mM NaCl results in a significant increase in fluorescence intensity of the particles (c, compare with Fig. 3e) suggesting that Na+ is transported into the porous spheres. Integration of the fluorescence intensities inside the particles before (f) and after (d) the increase of the bulk Na+ concentration shows that the average intensity increases by a factor of two. To show that gramicidin A-containing DLPC-bilayers are defect free and do not allow unrestricted passage of ions, an ionic quenching test of fluorescein by iodide was performed. Iodide is known to be an efficient quencher of fluorescence for fluorescein while it does not penetrate lipid bilayers in the fluid phase.41
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Fig. 3 Gramicidin-mediated uptake of Na+ into lipid bilayer-coated particles. (a) Schematic illustration. (b) A two-channel CLSM image of fluorescein-loaded particles sealed with a fluorescently labeled lipid bilayers containing 1 mol% of gramicidin A, (c) and (e) are the CLSM images of SG-loaded SNS particles (sealed with DLPC lipid bilayers containing 1 mol% of gramicidin A) with and without the addition of Na+ respectively, (d) and (f) are the respective histograms of the integral intensities per particle measured from the CLSM images. The data in (e) and (f) were obtained 48 hours after addition of Na+. Scale bars are 10 μm. |
We find that the fluorescence of the uncoated fluorescein-loaded SNS particles (Fig. 4a) is effectively quenched after addition of I− (b). The particles sealed with DLPC-gramicidin A bilayers (c) on the other hand did not show observable fluorescence quenching one hour after I− addition (d) indicating an ion-tight membrane and a Na+ selectivity for gramicidin A. This shows that the transport of Na+ into the DLPC-coated SNS illustrated in Fig. 3c is dominated by transport through the gramicidin A channels and that the transport through possible defects in the bilayer is insignificant. As a reference for unrestricted uptake, we find that adding 10 mM NaCl to unsealed SNS loaded with 10 μM of SG results in a 3-fold increase in the intensity (see Fig. S2, ESI†). In contrast, the fluorescence remained unchanged when a solution with the same concentration of Na+ was added to SG-loaded SNS coated with a pure DLPC lipid bilayer (no gramicidin) (see Fig. S3, ESI†). This process can also be reversed, i.e. DLPC-coated SNS preloaded with SG in Na+ buffer can release the Na+ ions through gramicidin A channels into a K+-containing (but Na+ free) buffer (Fig. 5).
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Fig. 4 Iodide quenching of fluorescein-loaded silica nanoporous spheres. Representative CLSM images of the fluorescein-loaded mesoporous silica particles; with coatings of gramicidin A-containing (1 mol%) DLPC lipid bilayers (c and d), and without any coating (a and b). Images recorded before (a and c) and after (b and d) addition of I− to the bulk media (final I− concentration 300 mM). The time indicated is the time after addition of I. |
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Fig. 5 Gramicidin-mediated release of Na+ from lipid bilayer-coated particles. CLSM images of monodisperse nanoporous silica spheres loaded with SG and 100 mM of Na+, and sealed with DLPC lipid bilayers containing 1 mol% of gramicidin A. The left panel shows a representative CLSM image and the histograms to the right show the integral intensities per particle (a) before, (b) after exchange of the bulk solution with Na+-containing fresh buffer (control sample) and (c) after exchange of the Na+-based with a K+-based bulk solution. Images in panels (b) and (c) were recorded 20 h after buffer exchange. The significant decrease in the fluorescence intensity after the addition of the K+-containing bulk solution in (c) shows that there is a significant uptake of potassium and release of sodium ions into/from the gramicidin containing lipid bilayer coated SNS. At the same time, unchanged fluorescence of the control sample (b) after 20 h shows that there are no major leaks. |
The fluorescence intensity after sodium uptake varies between individual particles. This is not surprising considering a spatial variation in the concentration and/or activity of the bilayer-bound gramicidin, variations in the pore volume and pore structure, both within and between particles, which is a known characteristic of porous spheres synthesized using the aerosol-assisted process,35 or by the different concentrations of the correctly oriented protein molecules in the lipid membrane of different particles.26
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Fig. 6 Schematic illustration of the ATP synthase incorporated into a lipid bilayer that covers a nanoporous particle loaded with SG. The ATP synthase comprises a membrane soluble F0 part that uses the Na+ gradient to rotate the F0 which subsequently generates a toque in the F1 part through a mechanical coupling between them. This conformational change results in a catalytic site for the reaction of ATP from ADP. In the reverse ATP hydrolysis mode, ATP is instead used up and ions are actively transported through the channel. |
Purified ATP synthase from I. tartaricus, heterogeneously expressed in E. coli was reconstituted in proteoliposomes. Functional reconstitution was verified by ATP synthesis measurements driven by a K+/valinomycin induced diffusion potential and a Na+-gradient (Fig. 7). The Na+ gradient is established by dispersing the proteoliposomes (loaded with 50 mM NaCl) into a solution containing 1 mM NaCl, while the electrical potential (inside positive) is created by valinomycin mediated K+ influx into the liposomes. Together, they build up a potential of approximately 230 mV, which is sufficient to initiate ATP synthesis.44 With time, the K+ concentration inside the liposomes rapidly increases and the electrical potential, and thus the ATP synthesis rate decreases.
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Fig. 7 Time dependent activity of the ATP synthase reconstituted in proteoliposomes. The synthesis of ATP by transportation of Na+ ions is measured after applying a K+/valinomycin induced diffusion potential and a Na+-gradient. |
The SNS particles were preloaded with SG before sealing with soy PC bilayers containing ATP synthase through liposomal fusion of reconstituted proteoliposomes. We have evaluated transmembrane transport of Na+ into membrane-sealed SNS particles by subjecting the particles to sodium ion solutions, and compared the uptake in the absence and the presence of ATP. Fig. 8 shows the change in fluorescence intensity (normalized to the intensity before adding Na2ATP or NaCl) over time for a selected number of particles. The stable fluorescence intensity in the control experiment with soy PC bilayer coated particles (without ATP synthase, Fig. 8a) shows that the lipid bilayer coating itself is ion-tight. Fig. 8b shows that the SG-loaded SNS particles sealed with soy PC bilayers that contain ATP synthase display a rapid increase in the fluorescence intensity of up to 60% when 0.4 mM Na2ATP is added to the bulk solution. The result shows a spread in the maximum uptake that is likely to be related to varying number of ATP synthase molecules per particle. A much smaller (∼20% increase in fluorescence intensity) uptake is also observed when the system is supplied with 4 mM NaCl in the absence of ATP (Fig. 8c). Hence, while the transport of Na+ into the lipid bilayer-coated SNS is dominated by ATP-driven transport, there is also a smaller passive Na+-influx in the absence of ATP. The rapid saturation of the intensity increase suggests that the passive transport is occurring through defective ATP synthases that lack the F1 head group after reconstitution, i.e. functioning as a passive channel that will transport Na+ ions due to the chemical gradient (4 mM outside, <200 μM inside). Indeed, dissociation of F1 from F0 leaving behind the two parts as separate functional entities, during reconstitution, has been reported previously.44
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Fig. 8 ATP synthase-mediated transport of Na+ into lipid bilayer-coated particles. Normalized intensity of fluorescence of SG-loaded porous silica spheres sealed by (a) only a soy PC bilayer after addition of 8 mM NaCl. Normalized intensity of fluorescence of SG-loaded porous silica spheres sealed by asoy PC bilayer containing 1 mol% ATP synthase after addition of (b) 0.4 mM Na2ATP, and (c) 4 mM NaCl. Specimens used in (b) and (c) were from the same batch and experimental conditions were kept the same. The first graph contains data for 5 spheres and the last 2 graphs contain data for 30 spheres. |
This versatile system allows for a solid and tunable platform for the utilization of large transmembrane proteins for both functional studies and biomimetic synthesis. It could for example be used with several different proteins, creating a chain reaction which further mimics the complex cascade reaction occurring in living cells. Also, it is envisaged that combinations of different ion transporters incorporated into supported lipid bilayers onto porous carriers could be used as biomimetic microreactors for controlled synthesis of inorganic multicomponent materials. A further uniqueness is that the membranes are supported by nanoporous particles, functioning as biomimetic proxies for cellular endoskeletons, which lends physical strength, dimensional stability and internal subdivision of space to these “protocells”.
The possibility of designing “protocells” with tunable porous endoskeletons offers a physically robust and biochemically versatile system, suitable for functional studies of complex membrane protein systems. Future prospects also include the exciting possibilities for biomimetic synthesis where membrane proteins control the transport of the ionic reactants into a nanoporous microreactor.
Footnotes |
† Electronic supplementary information (ESI) available: 1.1 Synthesis of nanoporous silica particles, 1.2 characterization of the monodisperse mesoporous spheres, Fig. S1 characterization of mesoporous silica particles. Fig. S2 CLSM scans of non-sealed particles before and after Na+ uptake, Fig. S3 CLSM images of the particles sealed with DLPC lipid bilayers without gramicidin A. See DOI: 10.1039/c2cp43166a |
‡ These authors contributed equally to this work. |
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