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. 2014 Aug 5;53(33):5384–5392. doi: 10.1021/bi500779g

Interaction of Daptomycin with Lipid Bilayers: A Lipid Extracting Effect

Yen-Fei Chen 1, Tzu-Lin Sun 1, Yen Sun 1, Huey W Huang 1,*
PMCID: PMC4148140  PMID: 25093761

Abstract

graphic file with name bi-2014-00779g_0009.jpg

Daptomycin is the first approved member of a new structural class of antibiotics, the cyclic lipopeptides. The peptide interacts with the lipid matrix of cell membranes, inducing permeability of the membrane to ions, but its molecular mechanism has been a puzzle. Unlike the ubiquitous membrane-acting host-defense antimicrobial peptides, daptomycin does not induce pores in the cell membranes. Thus, how it affects the permeability of a membrane to ions is not clear. We studied its interaction with giant unilamellar vesicles (GUVs) and discovered a lipid-extracting phenomenon that correlates with the direct action of daptomycin on bacterial membranes observed in a recent fluorescence microscopy study. Lipid extraction occurred only when the GUV lipid composition included phosphatidylglycerol and in the presence of Ca2+ ions, the same condition found to be necessary for daptomycin to be effective against bacteria. Furthermore, it occurred only when the peptide/lipid ratio exceeded a threshold value, which could be the basis of the minimal inhibitory concentration of daptomycin. In this first publication on the lipid extracting effect, we characterize its dependence on ions and lipid compositions. We also discuss possibilities for connecting the lipid extracting effect to the antibacterial activity of daptomycin.

Daptomycin (Figure 1) is an FDA (the U.S. Food and Drug Administration)-approved lipopeptide antibiotic, notably active against multidrug-resistant, Gram-positive pathogens, including methicillin-resistant Staphylococcus aureus (MRSA) and vancomycin-resistant Enterococcus (VRE). In recent reviews,1−3 it was concluded that despite nearly 25 years of study and 9 years of clinical use, aspects of the mechanism of action of daptomycin remained poorly understood. The evidence so far suggests that its main target is the cytoplasmic membrane, where daptomycin causes leakage of cations leading to loss of membrane potential and cell death.1,2,4−6 The membrane function is compromised in the absence of cell lysis or leakage of molecules other than atomic cations.6,7 What is not yet clear is what molecular process underlies the action of daptomycin. One major concern about the clinical use of daptomycin is the development of resistance during therapy. Many of the mutations that alter susceptibility to daptomycin have been shown to directly affect the membrane lipid composition.8−12 This further supports the role of the membrane being the central target for the action of daptomycin. Thus, the interaction of daptomycin with lipid bilayers is fundamental to its antibiotic activity.

Figure 1.

Figure 1

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Structural formula of daptomycin. The molecule has a net charge of approximately −3 at pH 7.

The antibacterial activity of daptomycin is calcium-dependent13 and correlates with the target membrane’s content of phosphatidylglycerol (PG).10 In the presence of Ca2+ ions, daptomycin spontaneously binds to artificial membranes,14 but only minor effects of daptomycin on lipid vesicles have been detected in past experiments.14−16 Fluorescence resonance energy transfer (FRET) experiments have shown daptomycin aggregation in membranes,17−19 but no leakage of calcein from lipid vesicles was detected.15 The only noticeable effect of daptomycin on the membrane properties was causing leakage of cations from lipid vesicles, but the effect was weak compared with that of an ionophore valinomycin at comparable concentrations.20 These earlier studies used artificial membranes in the form of small liposomes (≲100 nm).14−16,18,21 Here we used giant unilamellar vesicles (GUVs) (>10 μm) that allowed us to observe the action of daptomycin under a microscope. Our results are consistent with all previous measurements, but in addition, we discovered an effect of lipid extraction that appears to be similar to the direct action of daptomycin on bacterial membranes.1

Lipid extraction occurred only when the GUV lipid composition included phosphatidylglycerol (PG) and in the presence of Ca2+ ions, exactly the same condition found to be necessary for daptomycin to be effective against bacteria. The greatest advantage of the GUV method over the methods of smaller liposomes is that we can measure the membrane area change as daptomycin binds to it. Thus, we obtained a quantitative measure of the lipid extracting effect and showed that it has a daptomycin concentration dependence. We found that lipid extraction by daptomycin is a cooperative phenomenon with a threshold concentration. The effect was detected only for daptomycin concentrations above this threshold.

Because daptomycin targets bacterial cell membranes, the resistance mechanisms have been suspected to involve changes in the lipid composition of the bacterial cell membrane.9 One possibility is decreasing the extent of the synthesis of PG or increasing the extent of the conversion of PG to lysylphosphatidylglycerol (LPG).9 These were found in the resistant mutants of Staphylococcus aureus(22) and Bacillus subtilis.23 Our experiment shows that replacing PG with LPG has the effect of diminishing the lipid extracting effect. Another possibility involves cardiolipin.12 Recent reports suggested interference of cardiolipin with the action of daptomycin on membranes.24,25 Our experimental results described here are inadequate to address the reported effects of cardiolipin.

Materials and Methods

Materials

Daptomycin was purchased from Selleckchem (Munich, Germany) and from Haorui-Pharma Chem Inc. (Irvine, CA); 18:1 (Δ9-Cis) PC (DOPC), 18:1 (Δ9-Cis) PG (DOPG), 18:1 Liss Rhod PE (Rh-PE), 18:1 cardiolipin, and 18:1 Lysyl PG (lysyl PG) were purchased from Avanti Polar Lipids (Alabaster, AL). Texas Red sulfonyl chloride (MW 625) was purchased from Invitrogen Probe (Grand Island, NY). Fluorescence-labeled BODIPY-daptomycin was a gift from Cubist Pharmaceuticals, Inc. (Lexington, MA).

Aspirated GUV Experiment

This experiment was a modification of the original method of Kwok and Evans26 and of Longo et al.27 as described by Sun et al.28 Giant unilamellar vesicles (GUVs) of a chosen lipid composition were produced by the electroformation method29 in a solution containing 199 mM sucrose for the purpose of controlling the osmolality and 1 mM Tris (pH 7). Ten microliters of a GUV suspension was injected into a control chamber that contained 190 mM glucose and 10 mM Tris (pH 7). A selected GUV (diameter of ∼20–30 μm) was aspirated at a low constant negative pressure (∼100 Pa producing a membrane tension of ∼0.4 mN/m) with a micropipette, which was connected to an oil-filled U tube in which a negative pressure was produced and controlled by reference to the atmospheric pressure.28 A separate observation chamber contained ∼190 mM glucose, 10 mM Tris (pH 7), Ca2+ ions, and daptomycin. The aspirated GUV was then transferred through a movable pipe28 from the control chamber to the observation chamber. We used sucrose inside and glucose outside of GUV, so that GUVs sank to the bottom for ease of aspiration manipulation. Also the phase contrast between sucrose and glucose could be monitored by a phase condenser to detect possible leakage of sugar through the membrane. We included a small amount of dye lipid (1 mol % Rh-PE) to make the boundary of the GUV clear, except in the case of the dye leakage experiment in which 10 μM Texas Red sulfonyl chloride was encapsulated in the GUV. The osmolality of each solution used in the experiment was measured by the Wescor (Logan, UT) model 5520 vapor pressure osmometer. Equi-osmolality between the inside and outside of the GUV was the initial condition in all GUV experiments. The response of the GUV to daptomycin binding was observed and recorded by a camera-equipped microscope. All GUV experiments were performed at room temperature (∼25 °C).

The binding of daptomycin to a GUV can be monitored by the expansion of the membrane area. This expansion is too small to be measured accurately by the change in the diameter of GUV. We used a technique developed by Kwok and Evan,26 in which a spherical GUV was aspirated partially into a micropipette by a constant, low membrane tension (∼0.4 mN/m) (Figure 2A). The shape of the GUV then consisted of two parts, a spherical part and a cylindrical part, with different surface area/volume (A/V) ratios. An overall A/V change due to peptide binding would cause a repartition between these two parts, from which the change in area could be accurately measured. From the microscopic images, the length of the protrusion into the micropipette (Lp), the radius of the micropipette (Rp), and the radius of the GUV (Rv) were carefully measured. Then it is straightforward to show ΔA = 2πRpΔLp + 8πRvΔRv and ΔV = πRp2ΔLp + 4πRv2ΔRv.26 If there were no molecular leakage (see below) and as long as the inside and outside of the GUV had the same osmolality, there would be no change in volume. When ΔV = 0, ΔA is directly proportional to ΔLp: ΔA = 2πRp(1 – Rp/Rv)ΔLp. The fractional area change (ΔA/A) is calculated from the change in protrusion length ΔLp. When the protrusion length decreased, the data analysis was limited to the point at which the protrusion length vanished. The maximal negative ΔA/A value depended on the initial protrusion length (before the exposure to daptomycin) that varied from vesicle to vesicle. All experiments reported here were highly reproducible, although small quantitative variations were expected of GUV experiments. For the sake of clarity, only two or three representative results are presented in the figures for each type of experiment, approximately 20–30% of actual measurements. No error bars are shown because the results are interpreted qualitatively, except for the measurement of the threshold concentration.

Figure 2.

Figure 2

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Effect of daptomycin on 7/3 DOPC/DOPG GUVs (including 1% Rh-PE) in the presence of Ca2+ ions, in widefield images. (A) Rh-PE fluorescence widefield images of GUVs at different daptomycin concentrations (0.3, 1.0, and 5.0 μM from top to bottom, respectively). Note that the length of protrusion into the micropipette increased to a maximal value at 0.3 μM and increased and then decreased at 1.0 and 5.0 μM. When the protrusion length decreased, aggregates appear on the GUV surface. (B) Fractional area change ΔA/A of the GUVs over time. For the sake of clarity, only two or three representative runs are shown for each daptomycin concentration. The red data points and blue triangles ended when the GUV ruptured. (C) As ΔA/A decreased, substances including Rh-PE came off or appeared on the GUV surface, as indicated by arrows (see Movies S1 and S2 of the Supporting Information). The scale bar is 10 μm.

Results

Lipid Extracting Effect

The antibacterial activity of daptomycin requires Ca2+ ions.13 The standard media for in vitro susceptibility testing of daptomycin in clinical laboratories are set to a calcium content of 50 mg/L (∼1.25 mM),30 which is close to the calcium concentration in human serum.2 The reported minimal inhibitory concentration (MIC) values of daptomycin are in the micromolar range.2,13 Thus, we chose 1 μM daptomycin and 1 mM Ca2+ as our reference condition (we found our results to be insensitive to Ca2+ concentration from ∼0.5 to ∼2 mM). Also, the susceptibility of bacteria to daptomycin is correlated to the target membrane’s content of phosphatidylglycerol (PG).9,23 To simulate the PG content of bacterial membranes, we used lipid bilayers of a DOPC/DOPG mixture at a 7/3 ratio. PC/PG mixtures were commonly used in previous model membrane experiments15,17,18 for daptomycin.

First, for the control experiments, in the absence of daptomycin, we detected no membrane expansion of a 7/3 DOPC/DOPG GUV with Ca2+ (Figure S1 of the Supporting Information). Figure 2A shows the responses of the GUVs to the binding of daptomycin. The GUVs were made visible by including a small fraction (1 mol %) of 18:1 Liss Rhod PE (Rh-PE). They were transferred at time zero into an observation chamber containing a solution of daptomycin and Ca2+ ions (see Materials and Methods for the exact solution compositions). In a solution of 0.3 μM daptomycin, the peptide binding caused the GUV surface area to expand initially (see Figure 2B for ΔA/A values calculated from the increasing protrusion length ΔLp). Gradually, the area expansion saturated at a maximum ΔA/A value of ∼3% and showed no further changes. In contrast, when the daptomycin concentration was higher than 0.3 μM, the membrane area expansion first reached a maximum and then the area decreased (Figure 2). During the membrane area decrease, we detected lipid–peptide aggregates (see below) exuded from the outer surface of the GUV and most of the aggregates appeared to stay on the outer surface (Figure 2A,C). The phenomena are most clearly seen in the movies of the GUV images that show the movement of exuded substances (see Movies S1 and S2 of the Supporting Information). The aggregates were the end products of the reaction. The net effect on the GUV was that lipid molecules were removed or extracted from the lipid bilayer during the reaction and the amount of lipid in the GUV bilayer was reduced. Because the most important consequence of the interaction is the effect on the membrane, we will call this phenomenon the lipid extracting effect (see Note S1 of the Supporting Information).

To show that the aggregates are those of both lipid and daptomycin, we performed the same experiment with daptomycin, including 30% fluorescence-labeled BODIPY-daptomycin. (Note that BODIPY-daptomycin is 2–4 times less active than the unmodified molecule.1) Figure 3 shows that the exuded aggregates contained both Rh-PE and BODIPY-daptomycin.

Figure 3.

Figure 3

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Same experiment as in Figure 2 with fluorescent daptomycin shown as confocal images. A 7/3 DOPC/DOPG GUV (including 1% Rh-PE) was introduced at time zero into a solution containing 1 μM daptomycin with 0.5 μM BODIPY-daptomycin and 1 mM Ca2+. To show colocalization of lipid and peptide in aggregates, confocal images were taken: red for RH-PE and green for BODIPY-daptomycin. The GUV protrusion length increased and then decreased as in Figure 2. As the protrusion length decreased, aggregates appeared on the GUV surface containing both lipid and peptide. The scale bar is 10 μm.

To show that the protrusion length decrease was indeed due to lipid extraction, not caused, for example, by a GUV volume increase due to any exchange of solute between the inside and outside of the GUV,28,31 we performed a GUV (7/3 DOPC/DOPG) experiment with the inside and outside solutions being as similar as possible. We used an interior solution containing 1 mM pH 7.4 Tris buffer, 200 mM glucose, and 0.5 mM CaCl2 and an exterior solution containing 1 mM pH 7.4 Tris buffer, 200 mM glucose, 1.0 mM CaCl2, and 1 μM daptomycin. (GUVs are difficult to produce in 1.0 mM CaCl2.) Thus, the worst case leakage, if any, could at most affect the osmolality by 0.5%, which would change ΔA/A by at most ∼0.33%. The results shown in Figure 4 (and Movie S3 of the Supporting Information) are essentially the same as those shown in Figure 2 (compare with the data for 1 μM daptomycin); in both cases, ΔA/A decreased from a maximum by more than 4% that could be due to only lipid extraction.

Figure 4.

Figure 4

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DOPC/DOPG (7/3) GUVs containing 200 mM glucose, 1 mM pH 7.4 Tris buffer, and 0.5 mM CaCl2 were introduced, at time zero, into an observation chamber containing 200 mM glucose, 1 mM pH 7.4 Tris buffer, 1.0 mM CaCl2, and 1 μM daptomycin. The inside and outside solutions of GUV had equal osmolality as measured by an osmometer. Two runs are shown. The movie of one run is shown in Movie S3 of the Supporting Information. The scale bar is 10 μm.

Molecular Leakage Experiment

To test if the lipid extracting effect causes any molecular leakage, we included 10 μM Texas Red sulfonyl chloride (TRsc, MW 625) in the GUV. In this case, no dye lipid (Rh-PE) was used, because Lissamine Rhodamine B (Rh) and Texas Red are of the same color; consequently, the aggregates were not directly visible (Figure 5). The change in the slope of ΔA/A signaled the occurrence of lipid extraction, but there was no leakage of the content dye. The fluorescence intensity of the encapsulated TRsc decreased slightly over time at a rate comparable to that of photobleaching of the background fluorescence. For comparison, the TRsc leakage caused by melittin pores is shown in Figure S2 of the Supporting Information.

Figure 5.

Figure 5

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Molecular leakage experiment. A DOPC/DOPG (7/3) GUV encapsulating 10 μM TRsc was brought into a solution of 1 μM daptomycin and 1 mM Ca2+ at time zero, imaged by TRsc fluorescence. The increase and decrease in ΔA/A (scale on the right ordinate) indicates the occurrence of the lipid extracting effect (the aggregates are invisible for the lack of lipid dye). The intensity of TRsc fluorescence (scale on the left ordinate) inside the GUV (small circles) was the same as that of the control experiment (black line) without daptomycin, and both slowly decreased over time due to photobleaching. There was no leakage of TRsc of 625 MW during lipid extraction. For the sake of clarity, only one scan is shown. Another run is shown in Figure S2 of the Supporting Information where, for comparison, we also show a case of TRsc leakage by melittin pores. The scale bar is 10 μm.

Ion Dependence

What is the role of Ca2+ ions in the action of daptomycin on membranes? In the absence of Ca2+ ions, no binding of daptomycin was detected at a concentration of 1 μM (not shown). Even when Ca2+ was replaced with Mg2+ (at 1 mM), we saw little binding of daptomycin to the PG-containing membranes (Figure 6). This is consistent with the reports that the antibacterial activity of daptomycin requires Ca2+ ions13 and that the MICs increased at least 32-fold if Ca2+ ions were replaced with Mg2+ ions.21

Figure 6.

Figure 6

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Effect of daptomycin on 7/3 DOPC/DOPG GUVs in the absence of Ca2+. The top panel shows the GUV in 1 μM daptomycin and 1 mM Mg2+, in 5 μM daptomycin, and in 50 μM daptomycin (from top to bottom, respectively). The scale bar is 10 μm. The bottom panel shows the fractional area change ΔA/A of the GUVs over time. For the sake of clarity, only two representative runs are shown for each condition. There was no detectable binding of daptomycin at 1 μM, either with or without Mg2+ (not shown). However, even without Ca2+, daptomycin binds to DOPC/PG membranes at high concentrations (>5 μM).

However, if the daptomycin concentration was increased to 5 μM, there was a membrane area expansion indicating daptomycin binding at higher concentrations in the absence of Ca2+ ions. At 50 μM daptomycin without Ca2+ ions, the response of the GUV was similar to that with 1 μM daptomycin with Ca2+ (Figure 2). This result indicates that the role of Ca2+ is to facilitate the binding of daptomycin to lipid bilayers, as suggested in an earlier study,15 but the binding affinity of daptomycin for membranes is not zero in the absence of Ca2+. As long as there is a sufficient amount of daptomycin bound to a PG-containing membrane, there is a lipid extracting effect. Again, this is consistent with the MICs increasing 32-fold in the absence of Ca2+ ions.21

Lipid Dependence

The susceptibility of bacteria to daptomycin is correlated with the membrane content of PG.9 Indeed, we found that the lipid extracting effect occurred only when GUVs contained PG. Interestingly, daptomycin binds to the electrically neutral pure DOPC membrane in the presence of Ca2+ but exhibited no lipid extraction (Figure 7). The peptide moiety of daptomycin is anionic [net charge of approximately −3 at pH 7 (Figure 1)], yet it still has a low binding affinity for the DOPC/PG anionic lipid bilayer in the absence of Ca2+ (Figure 6). With Ca2+, daptomycin has a stronger affinity for DOPC than for DOPC mixed with anionic CL or LPG (Figure 7). Thus, the binding affinities of daptomycin for lipid bilayers do not follow a naive electrostatic argument based on the net charge.

Figure 7.

Figure 7

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Effect of daptomycin on GUVs in the absence of PG. (A) GUVs of pure DOPC, 7/1.5 DOPC/cardiolipin GUVs, and 7/3 DOPC/LPG GUVs (from top to bottom, respectively), all exposed to 1 μM daptomycin and 1 mM Ca2+. (The 7/1.5 DOPC/cardiolipin GUV was chosen to compare with the 7/3 DOPC/PG GUV because cardiolipin is a diphosphatidylglycerol lipid.) The lipid extracting effect was not seen in any of these experiments. The scale bar is 10 μm. (B) In each case, ΔA/A increased to a maximum without a decrease. For the sake of clarity, only two representative runs are shown for each experiment.

Some studies of the resistance to daptomycin implied the possibilities of shifting the phospholipid composition from PG to LPG in one case9,22,23 and to CL in another.11,12 We found that replacing PG with either LPG or CL eliminated the lipid extracting effect at a daptomycin concentration of 1 μM (Figure 7). However, the most recent studies implied possible interference of CL with the action of daptomycin.24,25 This clearly calls for much more extensive studies of daptomycin with the lipid mixtures of CL and PG.

Existence of a Threshold Concentration

The lipid extracting effect has a strong daptomycin concentration dependence. Below a threshold concentration, the effect was absent. Above the threshold, the effect occurred in a shorter and shorter time as the daptomycin concentration increased. To quantify this dependence, we plotted the time τ for reaching the maximum of ΔA/A [(ΔA/A)max] as a function of daptomycin concentration (Figure 8). As the daptomycin concentration decreased from 4 to 0.4 μM, the time to reach (ΔA/A)max exponentially increased. When the concentration decreased to 0.3 μM, the membrane area increased to ∼3% and stayed constant without a decrease (Figure 2); there was no lipid extracting effect, equivalent to τ → ∞. Thus, the threshold concentration for the lipid extracting effect is ∼0.3 μM or, more exactly, between 0.3 and 0.4 μM. These measurements were first performed at a constant Ca2+ concentration of 1.25 mM. The same result was reproduced at 0.5 and 1.0 mM Ca2+ (Figure 8).

Figure 8.

Figure 8

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Time τ to the maximal ΔA/A [(ΔA/A)max] vs daptomycin concentration. The Ca2+ concentration was constant at 1.25, 1.0, and 0.5 mM (from top to bottom, respectively). The inset shows examples of how τ was measured for 1 and 2 μM daptomycin (see arrows). The curves are a guide to the eye. The vertical dashed lines are at 0.3 μM. The error bars represent the ranges of reproducibility by several runs. The results measured at three different Ca2+ concentrations are essentially the same.

We examined all GUV experiments with a 7/3 DOPC/DOPG GUV and Ca2+ ions and concluded that there is a critical value of (ΔA/A)max of ∼3%. [This is the average of (ΔA/A)max values for daptomycin at 0.4–0.5 μM.] At <0.4 μM daptomycin, ΔA/A reaches a constant value of ≲3% without a lipid extracting effect. At >0.4 μM daptomycin, ΔA/A increases to a (ΔA/A)max of >3% and then decreases, concurrent with a lipid extracting effect. The lipid extracting effect started when the membrane expansion ΔA/A reached the critical value of ∼3%. However, at high daptomycin concentrations, the membrane area continued to increase even after the lipid extracting effect had started, because daptomycin continued to bind to the lipid bilayer from the solution. Consequently, the (ΔA/A)max value could reach ∼6% before the membrane area started to decrease showing the effect of lipid extraction (Figure 2B).

Discussion

Daptomycin is the first approved member of a new structural class of antibiotics, the cyclic lipopeptides (Figure 1). It is a water-soluble membrane-acting antibiotic.1,2,4−6 The apparent membrane-acting feature of the molecule is its hydrophobic N-terminal decanoyl chain. It is worth noting that the decanoyl chain can be replaced by varieties of hydrophobic substitutes without losing antibacterial activity.18,32 The hydrophobic moiety is expected to insert into the hydrocarbon region of a membrane. However, the research so far has not yielded the molecular configuration of membrane-bound daptomycin. There is a change in the circular dichroism (CD)15 of daptomycin when it binds to PG-containing lipid bilayers in the presence of Ca2+, indicating a possible structural change upon membrane binding, but there has been no theoretical interpretation of the CD spectra of daptomycin. Nuclear magnetic resonance studies were limited to daptomycin in solutions without lipid bilayers.15,33,34 The lack of structural information about membrane-bound daptomycin is the main obstacle for understanding its molecular mechanism.

Over the past two and a half decades, the field of membrane-active peptides has grown from the studies of host-defense antimicrobial peptides (AMPs).35−41 AMPs are characterized by their abilities to form pores in membranes and cause leakage of dye molecules from lipid vesicles.35−41 Thus, very active research of AMPs has focused on the molecular mechanisms of AMPs that cause molecular leakage.35−41 In contrast, daptomycin does not induce molecular leakage across a membrane;6,7 the proof is shown here in Figure 5 (and Figure S2 of the Supporting Information; see Note S2 of the Supporting Information). Compared with the research publications for AMPs, there are fewer studies of daptomycin–membrane interactions because of the lack of obvious effects on the membrane. Until now, the only detected reaction in membranes is oligomerization or aggregation of daptomycin by the FRET technique.17,18 A hypothesis for transmembrane octameric daptomycin pores has been postulated from the FRET and ion leakage experiments.19,20,25 This hypothesis required many assumptions19,20,25 that have not been critically evaluated. There is no structural evidence of such pores, and there are no free energy arguments about why daptomycin, given its molecular structure, would form such an octameric complex and why such a complex would be stable inside a lipid bilayer. In contrast, pores induced by AMPs have been detected by X-ray diffraction in lipid crystallines41,42 and by neutron scattering in fluid membranes,43,44 and they are free energy minimum states (see references in refs (40) and (41)).

Here we discovered an effect of daptomycin on lipid bilayers that appeared to be similar to the direct action of daptomycin on bacterial membranes observed in a recent fluorescence microscopy study,1 i.e., inducing lipid aggregates on the surface of a bacterial membrane. We emphasize that the observed aggregates are the end product of the daptomycin interaction. We imagine that the aggregates must have started from a microscopic size and became visible only after they grew or combine to micrometer size. With a microscope, we cannot see the aggregation process. Most of the macroscopic aggregates appeared to stay on the GUV surface. They moved away from the GUV surface if there was a flow in the solution (see Movies S1 and S2 of the Supporting Information). As far as we could detect, the aggregates staying on the surface of GUV had no effect on the property of the GUV bilayer. Therefore, we believe that the main effect of daptomycin on the membrane is removing lipid molecules from the bilayers as a result of the interaction.

The lipid extracting effect is a predictable reaction of daptomycin with lipid bilayers under specific conditions. It occurred only when the GUV lipid composition included PG and in the presence of Ca2+ ions, the same condition found to be necessary for daptomycin to be effective against bacteria.10,13 Most surprisingly, the lipid extracting effect has an all-or-none cooperative concentration dependence that is similarly to a MIC. This suggests that the lipid extracting effect and the antibacterial activity of daptomycin are correlated. The current consensus view of daptomycin’s bactericidal activity is that it causes leakage of atomic cations through the cytoplasmic membrane of bacteria, leading to loss of membrane potential and cell death.1,2,4−6 It compromises the membrane function without cell lysis or molecular leakage.6,7 Can the lipid extracting effect be the underlying mechanism for the bactericidal activity? We discuss this possibility by offering the following observations.

Lipid Extraction and Ion Leakage

The permeation of a membrane by ions is one of the subjects most studied by molecular simulations.45−49 The consensus results can be summarized as follows. (i) Ion permeation is an activated process; spontaneous ion permeation is rare.48,49 (ii) Ions enter the bilayer with a trail of water molecules called water fingers45 (the potential energy for an isolated ion in membrane is too high). The water finger is lined by lipid headgroups. This results in a major rearrangement of neighboring lipids, commonly called water pore defects.45−49 (iii) Simulations by displacing a pair of chain-to-chain lipid molecules from a bilayer create a water pore defect, allowing ion permeation.47 (iv) The transient water pores created by activated ion permeation or by lipid molecule displacement have radii of <1 nm46 and lifetimes of 10–100 ns.46,47

Thus, it is reasonable to expect that daptomycin-induced lipid extraction can lead to ion permeation. So far, daptomycin-induced K+4 and Mg2+6 leakage has been observed in bacteria. The negative counterions were most likely blocked from permeation by the presence of anionic lipid PG. The water pore defects induced by the lipid extracting effect would be too transient and too small to allow molecular leakage. It is well-known that very small amounts of net charge translocation can cause significant changes in membrane potential; e.g., it has been demonstrated that the translocation of only 2.9 × 103 H+ ions per Escherichia coli cell was sufficient to change the membrane potential by 16 mV.50,51

Molecular Process That Causes Lipid Extraction

The lipid extraction effect is not unique to daptomycin. Similar effects have been observed previously in the studies of β-amyloid peptides human islet amyloid polypeptide (hIAPP)52 and amyloidogenic peptide penetratin.53,54 Despite having different molecular structures, daptomycin and β-amyloid peptides exhibit similar behaviors in solution. β-Amyloid peptides are monomeric at low concentrations but aggregate at high concentrations.55 Similarly, daptomycin exists as soluble monomers at micromolar concentrations17 but oligmerizes at millimolar concentrations.15,21,33

In the presence of lipid bilayers, β-amyloid peptides first bind to bilayers as α-helical monomers, but when the bound peptide/lipid ratio exceeds a threshold, peptides transform from α-monomers to β-sheet aggregates (can be detected by CD).52−54 The latter appeared as peptide–lipid aggregates on the membrane surface,52,53 exactly like the aggregates induced by daptomycin. Normally, a molecule bound to a lipid bilayer either adsorbs on the interface between the headgroups and the chains or embeds inside the chain region. Both the β-peptide aggregates and the daptomycin aggregates unbind from the lipid bilayer, because, we believe, they are not compatible with being a bound state in lipid bilayers. It is not clear in either case whether lipid is intrinsically part of the molecular aggregation or lipid molecules attach to the peptide aggregates when the latter unbind from the bilayer. In either case, the actions of molecular aggregation and unbinding from the bilayer have an effect of lipid extraction, i.e., removing lipid molecules from the bilayer.

The connection of the lipid extracting effect to daptomycin’s bactericidal activity is reinforced by the findings that hIAPP and penetratin are cytotoxic56,57 and antibacterial,58,59 respectively. They were also found to induce transmembrane ion conduction without causing molecular leakage.53,54,60−65

Acknowledgments

We thank Cubist Pharmaceuticals, Inc., for providing BIDOPY-daptomycin.

Supporting Information Available

Movies of Figure 2 showing the effect of daptomycin on 7/3 DOPC/DOPG GUVs (including 1% Rh-PE) in the presence of Ca2+ ions (Movies 1 and 2), movie of Figure 4 showing the lipid extracting effect when the inside and outside solutions of the GUV are almost the same (Movie S3), control experiments without daptomycin (Figure S1), additional runs of the molecular leakage experiment as shown in Figure 5 (Figure S2), and additional notes and references. This material is available free of charge via the Internet at http://pubs.acs.org.

This work was supported by National Institutes of Health Grant GM55203 and Robert A. Welch Foundation Grant C-0991.

The authors declare no competing financial interest.

Funding Statement

National Institutes of Health, United States

Supplementary Material

bi500779g_si_001.pdf (357.2KB, pdf)
bi500779g_si_002.avi (974.9KB, avi)
bi500779g_si_003.avi (167.3KB, avi)
bi500779g_si_004.avi (132.3KB, avi)

References

  1. Pogliano J.; Pogliano N.; Silverman J. A. (2012) Daptomycin-mediated reorganization of membrane architecture causes mislocalization of essential cell division proteins. J. Bacteriol. 194, 4494–4504. [DOI] [PMC free article] [PubMed] [Google Scholar]
  2. Cottagnoud P. (2008) Daptomycin: A new treatment for insidious infections due to Gram-positive pathogens. Swiss Med. Wkly. 138, 93–99. [DOI] [PubMed] [Google Scholar]
  3. Vilhena C.; Bettencourt A. (2012) Daptomycin: A review of properties, clinical use, drug delivery and resistance. Mini-Rev. Med. Chem. 12, 202–209. [DOI] [PubMed] [Google Scholar]
  4. Silverman J. A.; Perlmutter N. G.; Shapiro H. M. (2003) Correlation of daptomycin bactericidal activity and membrane depolarization in Staphylococcus aureus. Antimicrob. Agents Chemother. 47, 2538–2544. [DOI] [PMC free article] [PubMed] [Google Scholar]
  5. Mascio C. T.; Alder J. D.; Silverman J. A. (2007) Bactericidal action of daptomycin against stationary-phase and nondividing Staphylococcus aureus cells. Antimicrob. Agents Chemother. 51, 4255–4260. [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Hobbs J. K.; Miller K.; O’Neill A. J.; Chopra I. (2008) Consequences of daptomycin-mediated membrane damage in Staphylococcus aureus. J. Antimicrob. Chemother. 62, 1003–1008. [DOI] [PubMed] [Google Scholar]
  7. Cotroneo N.; Harris R.; Perlmutter N.; Beveridge T.; Silverman J. A. (2008) Daptomycin exerts bactericidal activity without lysis of Staphylococcus aureus. Antimicrob. Agents Chemother. 52, 2223–2225. [DOI] [PMC free article] [PubMed] [Google Scholar]
  8. Arias C. A.; Panesso D.; McGrath D. M.; Qin X.; Mojica M. F.; Miller C.; Diaz L.; Tran T. T.; Rincon S.; Barbu E. M.; Reyes J.; Roh J. H.; Lobos E.; Sodergren E.; Pasqualini R.; Arap W.; Quinn J. P.; Shamoo Y.; Murray B. E.; Weinstock G. M. (2011) Genetic basis for in vivo daptomycin resistance in enterococci. N. Engl. J. Med. 365, 892–900. [DOI] [PMC free article] [PubMed] [Google Scholar]
  9. Friedman L.; Alder J. D.; Silverman J. A. (2006) Genetic changes that correlate with reduced susceptibility to daptomycin in Staphylococcus aureus. Antimicrob. Agents Chemother. 50, 2137–2145. [DOI] [PMC free article] [PubMed] [Google Scholar]
  10. Hachmann A. B.; Sevim E.; Gaballa A.; Popham D. L.; Antelmann H.; Helmann J. D. (2011) Reduction in membrane phosphatidylglycerol content leads to daptomycin resistance in Bacillus subtilis. Antimicrob. Agents Chemother. 55, 4326–4337. [DOI] [PMC free article] [PubMed] [Google Scholar]
  11. Palmer K. L.; Daniel A.; Hardy C.; Silverman J.; Gilmore M. S. (2011) Genetic basis for daptomycin resistance in enterococci. Antimicrob. Agents Chemother. 55, 3345–3356. [DOI] [PMC free article] [PubMed] [Google Scholar]
  12. Davlieva M.; Zhang W.; Arias C. A.; Shamoo Y. (2013) Biochemical characterization of cardiolipin synthase mutations associated with daptomycin resistance in enterococci. Antimicrob. Agents Chemother. 57, 289–296. [DOI] [PMC free article] [PubMed] [Google Scholar]
  13. Barry A. L.; Fuchs P. C.; Brown S. D. (2001) In vitro activities of daptomycin against 2,789 clinical isolates from 11 North American medical centers. Antimicrob. Agents Chemother. 45, 1919–1922. [DOI] [PMC free article] [PubMed] [Google Scholar]
  14. Jung D.; Powers J. P.; Straus S. K.; Hancock R. E. (2008) Lipid-specific binding of the calcium-dependent antibiotic daptomycin leads to changes in lipid polymorphism of model membranes. Chem. Phys. Lipids 154, 120–128. [DOI] [PubMed] [Google Scholar]
  15. Jung D.; Rozek A.; Okon M.; Hancock R. E. (2004) Structural transitions as determinants of the action of the calcium-dependent antibiotic daptomycin. Chem. Biol. 11, 949–957. [DOI] [PubMed] [Google Scholar]
  16. Straus S. K.; Hancock R. E. (2006) Mode of action of the new antibiotic for Gram-positive pathogens daptomycin: Comparison with cationic antimicrobial peptides and lipopeptides. Biochim. Biophys. Acta 1758, 1215–1223. [DOI] [PubMed] [Google Scholar]
  17. Muraih J. K.; Pearson A.; Silverman J.; Palmer M. (2011) Oligomerization of daptomycin on membranes. Biochim. Biophys. Acta 1808, 1154–1160. [DOI] [PubMed] [Google Scholar]
  18. Muraih J. K.; Harris J.; Taylor S. D.; Palmer M. (2012) Characterization of daptomycin oligomerization with perylene excimer fluorescence: Stoichiometric binding of phosphatidylglycerol triggers oligomer formation. Biochim. Biophys. Acta 1818, 673–678. [DOI] [PubMed] [Google Scholar]
  19. Muraih J. K.; Palmer M. (2012) Estimation of the subunit stoichiometry of the membrane-associated daptomycin oligomer by FRET. Biochim. Biophys. Acta 1818, 1642–1647. [DOI] [PubMed] [Google Scholar]
  20. Zhang T.; Muraih J. K.; MacCormick B.; Silverman J.; Palmer M. (2014) Daptomycin forms cation- and size-selective pores in model membranes. Biochim. Biophys. Acta 1838, 2425–2430. [DOI] [PubMed] [Google Scholar]
  21. Ho S. W.; Jung D.; Calhoun J. R.; Lear J. D.; Okon M.; Scott W. R.; Hancock R. E.; Straus S. K. (2008) Effect of divalent cations on the structure of the antibiotic daptomycin. Eur. Biophys. J. 37, 421–433. [DOI] [PubMed] [Google Scholar]
  22. Jones T.; Yeaman M. R.; Sakoulas G.; Yang S. J.; Proctor R. A.; Sahl H. G.; Schrenzel J.; Xiong Y. Q.; Bayer A. S. (2008) Failures in clinical treatment of Staphylococcus aureus infection with daptomycin are associated with alterations in surface charge, membrane phospholipid asymmetry, and drug binding. Antimicrob. Agents Chemother. 52, 269–278. [DOI] [PMC free article] [PubMed] [Google Scholar]
  23. Hachmann A. B.; Angert E. R.; Helmann J. D. (2009) Genetic analysis of factors affecting susceptibility of Bacillus subtilis to daptomycin. Antimicrob. Agents Chemother. 53, 1598–1609. [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Tran T. T.; Panesso D.; Mishra N. N.; Mileykovskaya E.; Guan Z.; Munita J. M.; Reyes J.; Diaz L.; Weinstock G. M.; Murray B. E.; Shamoo Y.; Dowhan W.; Bayer A. S.; Arias C. A. (2013) Daptomycin-resistant Enterococcus faecalis diverts the antibiotic molecule from the division septum and remodels cell membrane phospholipids. MBio 4, e00281-13. [DOI] [PMC free article] [PubMed] [Google Scholar]
  25. Zhang T.; Muraih J. K.; Tishbi N.; Herskowitz J.; Victor R. L.; Silverman J.; Uwumarenogie S.; Taylor S. D.; Palmer M.; Mintzer E. (2014) Cardiolipin prevents membrane translocation and permeabilization by daptomycin. J. Biol. Chem. 289, 11584–11591. [DOI] [PMC free article] [PubMed] [Google Scholar]
  26. Kwok R.; Evans E. (1981) Thermoelasticity of large lecithin bilayer vesicles. Biophys. J. 35, 637–652. [DOI] [PMC free article] [PubMed] [Google Scholar]
  27. Longo M. L.; Waring A. J.; Gordon L. M.; Hammer D. A. (1998) Area expansion and permeation of phospholipid membrane bilayer by influenza fusion peptides and melittin. Langmuir 14, 2385–2395. [Google Scholar]
  28. Sun Y.; Hung W. C.; Chen F. Y.; Lee C. C.; Huang H. W. (2009) Interaction of tea catechin (−)-epigallocatechin gallate with lipid bilayers. Biophys. J. 96, 1026–1035. [DOI] [PMC free article] [PubMed] [Google Scholar]
  29. Angelova M. I. (2000) Liposome Electroformation. In Giant Vesicles (Luisi P. L., and Walde P., Eds.) pp 27–36, John Wiley & Sons, Chichester, U.K. [Google Scholar]
  30. Fuchs P. C.; Barry A. L.; Brown S. D. (2000) Daptomycin susceptibility tests: Interpretive criteria, quality control, and effect of calcium on in vitro tests. Diagn. Microbiol. Infect. Dis. 38, 51–58. [DOI] [PubMed] [Google Scholar]
  31. Lee M. T.; Hung W. C.; Chen F. Y.; Huang H. W. (2008) Mechanism and kinetics of pore formation in membranes by water-soluble amphipathic peptides. Proc. Natl. Acad. Sci. U.S.A. 105, 5087–5092. [DOI] [PMC free article] [PubMed] [Google Scholar]
  32. Debono M.; Abbott B. J.; Molloy R. M.; Fukuda D. S.; Hunt A. H.; Daupert V. M.; Counter F. T.; Ott J. L.; Carrell C. B.; Howard L. C.; et al. (1988) Enzymatic and chemical modifications of lipopeptide antibiotic A21978C: The synthesis and evaluation of daptomycin (LY146032). J. Antibiot. 41, 1093–1105. [DOI] [PubMed] [Google Scholar]
  33. Ball L. J.; Goult C. M.; Donarski J. A.; Micklefield J.; Ramesh V. (2004) NMR structure determination and calcium binding effects of lipopeptide antibiotic daptomycin. Org. Biomol. Chem. 2, 1872–1878. [DOI] [PubMed] [Google Scholar]
  34. Rotondi K. S.; Gierasch L. M. (2005) A well-defined amphipathic conformation for the calcium-free cyclic lipopeptide antibiotic, daptomycin, in aqueous solution. Biopolymers 80, 374–385. [DOI] [PubMed] [Google Scholar]
  35. Boman H. G., Marsh J., and Goode J. A., Eds. (1994) Antimicrobial peptides, Vol. 186, John Wiley & Sons, Chichester, U.K. [Google Scholar]
  36. Shai Y. (1999) Mechanism of the binding, insertion and destabilization of phospholipid bilayer membranes by α-helical antimicrobial and cell non-selective membrane-lytic peptides. Biochim. Biophys. Acta 1462, 55–70. [DOI] [PubMed] [Google Scholar]
  37. Matsuzaki K. (1998) Magainins as paradigm for the mode of action of pore forming polypeptides. Biochim. Biophys. Acta 1376, 391–400. [DOI] [PubMed] [Google Scholar]
  38. Huang H. W. (2000) Action of antimicrobial peptides: Two-state model. Biochemistry 39, 8347–8352. [DOI] [PubMed] [Google Scholar]
  39. Zasloff M. (2002) Antimicrobial peptides of multicellular organisms. Nature 415, 389–395. [DOI] [PubMed] [Google Scholar]
  40. Last N. B.; Miranker A. D. (2013) Common mechanism unites membrane poration by amyloid and antimicrobial peptides. Proc. Natl. Acad. Sci. U.S.A. 110, 6382–6387. [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Lee M. T.; Sun T. L.; Hung W. C.; Huang H. W. (2013) Process of inducing pores in membranes by melittin. Proc. Natl. Acad. Sci. U.S.A. 110, 14243–14248. [DOI] [PMC free article] [PubMed] [Google Scholar]
  42. Qian S.; Wang W.; Yang L.; Huang H. W. (2008) Structure of transmembrane pore induced by Bax-derived peptide: Evidence for lipidic pores. Proc. Natl. Acad. Sci. U.S.A. 105, 17379–17383. [DOI] [PMC free article] [PubMed] [Google Scholar]
  43. Ludtke S. J.; He K.; Heller W. T.; Harroun T. A.; Yang L.; Huang H. W. (1996) Membrane pores induced by magainin. Biochemistry 35, 13723–13728. [DOI] [PubMed] [Google Scholar]
  44. Yang L.; Harroun T. A.; Weiss T. M.; Ding L.; Huang H. W. (2001) Barrel-stave model or toroidal model? A case study on melittin pores. Biophys. J. 81, 1475–1485. [DOI] [PMC free article] [PubMed] [Google Scholar]
  45. Benjamin I. (1993) Mechanism and dynamics of ion transfer across a liquid-liquid interface. Science 261, 1558–1560. [DOI] [PubMed] [Google Scholar]
  46. Gurtovenko A. A.; Vattulainen I. (2007) Ion leakage through transient water pores in protein-free lipid membranes driven by transmembrane ionic charge imbalance. Biophys. J. 92, 1878–1890. [DOI] [PMC free article] [PubMed] [Google Scholar]
  47. Tieleman D. P.; Marrink S. J. (2006) Lipids out of equilibrium: Energetics of desorption and pore mediated flip-flop. J. Am. Chem. Soc. 128, 12462–12467. [DOI] [PubMed] [Google Scholar]
  48. Tepper H. L.; Voth G. A. (2006) Mechanisms of passive ion permeation through lipid bilayers: Insights from simulations. J. Phys. Chem. B 110, 21327–21337. [DOI] [PMC free article] [PubMed] [Google Scholar]
  49. Khavrutskii I. V.; Gorfe A. A.; Lu B.; McCammon J. A. (2009) Free energy for the permeation of Na+ and Cl– ions and their ion-pair through a zwitterionic dimyristoyl phosphatidylcholine lipid bilayer by umbrella integration with harmonic fourier beads. J. Am. Chem. Soc. 131, 1706–1716. [DOI] [PMC free article] [PubMed] [Google Scholar]
  50. Cecchini G.; Koch A. L. (1975) Effect of uncouplers on “downhill” β-galactoside transport in energy-depleted cells of Escherichia coli. J. Bacteriol. 123, 187–195. [DOI] [PMC free article] [PubMed] [Google Scholar]
  51. Gould J. M.; Cramer W. A. (1977) Relationship between oxygen-induced proton efflux and membrane energization in cells of Escherichia coli. J. Biol. Chem. 252, 5875–5882. [PubMed] [Google Scholar]
  52. Lee C. C.; Sun Y.; Huang H. W. (2012) How type II diabetes-related islet amyloid polypeptide damages lipid bilayers. Biophys. J. 102, 1059–1068. [DOI] [PMC free article] [PubMed] [Google Scholar]
  53. Lee C. C.; Sun Y.; Huang H. W. (2010) Membrane-mediated peptide conformation change from α-monomers to β-aggregates. Biophys. J. 98, 2236–2245. [DOI] [PMC free article] [PubMed] [Google Scholar]
  54. Sun Y.; Lee C. C.; Chen T. H.; Huang H. W. (2010) Kinetic Process of β-Amyloid Formation via Membrane Binding. Biophys. J. 99, 544–552. [DOI] [PMC free article] [PubMed] [Google Scholar]
  55. Jarrett J. T.; Lansbury P. T. Jr. (1993) Seeding “one-dimensional crystallization” of amyloid: A pathogenic mechanism in Alzheimer’s disease and scrapie?. Cell 73, 1055–1058. [DOI] [PubMed] [Google Scholar]
  56. Haataja L.; Gurlo T.; Huang C. J.; Butler P. C. (2008) Islet amyloid in type 2 diabetes, and the toxic oligomer hypothesis. Endocr. Rev. 29, 303–316. [DOI] [PMC free article] [PubMed] [Google Scholar]
  57. Konarkowska B.; Aitken J. F.; Kistler J.; Zhang S.; Cooper G. J. (2006) The aggregation potential of human amylin determines its cytotoxicity towards islet β-cells. FEBS J. 273, 3614–3624. [DOI] [PubMed] [Google Scholar]
  58. Garro A. D.; Olivella M. S.; Bombasaro J. A.; Lima B.; Tapia A.; Feresin G.; Perczel A.; Somlai C.; Penke B.; Lopez Cascales J.; Rodriguez A. M.; Enriz R. D. (2013) Penetratin and Derivatives Acting as Antibacterial Agents. Chem. Biol. Drug Des. 82, 167–177. [DOI] [PubMed] [Google Scholar]
  59. Bahnsen J. S.; Franzyk H.; Sandberg-Schaal A.; Nielsen H. M. (2013) Antimicrobial and cell-penetrating properties of penetratin analogs: Effect of sequence and secondary structure. Biochim. Biophys. Acta 1828, 223–232. [DOI] [PubMed] [Google Scholar]
  60. Janson J.; Ashley R. H.; Harrison D.; McIntyre S.; Butler P. C. (1999) The mechanism of islet amyloid polypeptide toxicity is membrane disruption by intermediate-sized toxic amyloid particles. Diabetes 48, 491–498. [DOI] [PubMed] [Google Scholar]
  61. Anguiano M.; Nowak R. J.; Lansbury P. T. Jr. (2002) Protofibrillar islet amyloid polypeptide permeabilizes synthetic vesicles by a pore-like mechanism that may be relevant to type II diabetes. Biochemistry 41, 11338–11343. [DOI] [PubMed] [Google Scholar]
  62. Kayed R.; Sokolov Y.; Edmonds B.; McIntire T. M.; Milton S. C.; Hall J. E.; Glabe C. G. (2004) Permeabilization of lipid bilayers is a common conformation-dependent activity of soluble amyloid oligomers in protein misfolding diseases. J. Biol. Chem. 279, 46363–46366. [DOI] [PubMed] [Google Scholar]
  63. Quist A.; Doudevski I.; Lin H.; Azimova R.; Ng D.; Frangione B.; Kagan B.; Ghiso J.; Lal R. (2005) Amyloid ion channels: A common structural link for protein-misfolding disease. Proc. Natl. Acad. Sci. U.S.A. 102, 10427–10432. [DOI] [PMC free article] [PubMed] [Google Scholar]
  64. Kawahara M.; Kuroda Y.; Arispe N.; Rojas E. (2000) Alzheimer’s β-amyloid, human islet amylin, and prion protein fragment evoke intracellular free calcium elevations by a common mechanism in a hypothalamic GnRH neuronal cell line. J. Biol. Chem. 275, 14077–14083. [DOI] [PubMed] [Google Scholar]
  65. Mirzabekov T. A.; Lin M. C.; Kagan B. L. (1996) Pore formation by the cytotoxic islet amyloid peptide amylin. J. Biol. Chem. 271, 1988–1992. [DOI] [PubMed] [Google Scholar]

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