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Kinetic study of membrane protein interactions: from
three to two dimensions

Vladimir Adrien, Nicolas Taulier, Alice Verchère, Laura Monlezun, Martin Picard, Arnaud Ducruix, Isabelle Broutin, Frédéric Pincet, Wladimir Urbach

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Vladimir Adrien, Nicolas Taulier, Alice Verchère, Laura Monlezun, Martin Picard, et al. Kinetic study of membrane protein interactions: from three to two dimensions. Scientific Reports, 2024, 14 (1), pp.882. 10.1038/s41598-023-50827-5. hal-04450038

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# Kinetic study of membrane protein interactions: from three to two dimensions

Vladimir Adrien<fnref n="1" />,²,³✉, Nicolas Taulier⁴, Alice Verchère⁵, Laura Monlezun⁶, Martin Picard⁷,⁸, Arnaud Ducruix⁵, Isabelle Broutin⁵, Frédéric Pincet<fnref n="1" />✉ & Wladimir Urbach<fnref n="1" />,⁴✉

Molecular interactions are contingent upon the system's dimensionality. Notably, comprehending the impact of dimensionality on protein-protein interactions holds paramount importance in foreseeing protein behaviour across diverse scenarios, encompassing both solution and membrane environments. Here, we unravel interactions among membrane proteins across various dimensionalities by quantifying their binding rates through fluorescence recovery experiments. Our findings are presented through the examination of two protein systems: streptavidin-biotin and a protein complex constituting a bacterial efflux pump. We present here an original approach for gauging a two-dimensional binding constant between membrane proteins embedded in two opposite membranes. The quotient of protein binding rates in solution and on the membrane represents a metric denoting the exploration distance of the interacting sites—a novel interpretation.

Understanding the strength of protein interactions within disease pathways informs the design of drugs aimed at disrupting these interactions and impeding disease progression. The interactions among proteins are notably influenced by the surrounding space's availability, which corresponds to its dimensionality. This dependence on dimensionality arises from the system's geometry, which directly shapes the degrees of freedom and thereby influences interaction characteristics.

In lipid bilayers, proteins that interact within the same bilayer (cis interactions) or between distinct bilayers (trans interactions) can undergo either attractive or repulsive forces according to the charges of neighboring proteins or the surrounding lipid head groups. In three-dimensional systems such as the cytoplasm or extracel-lular space, interactions among proteins are influenced by a greater number of degrees of freedom compared to bilayers, given their enhanced ability to move and rotate. A scenario of intermediate significance arises when a membrane-bound protein interacts with a soluble counterpart, a common occurrence within cells. Additionally, the system's dimensionality can undergo alteration during protein-protein interactions; for instance, proteins interacting within the cytoplasm might become anchored to the plasma membrane, leading to a shift in the system's geometry and potentially modifying the strength and nature of their interactions<fnref n="1" />⁻⁵.

Despite this reality, most prevalent approaches tend to disregard these complexities. They typically examine the interaction of soluble proteins in solution and membrane proteins integrated into supported bilayers or micellar systems designed for soluble proteins⁶⁻⁸. Nonetheless, a few techniques permit a direct comparison of interactions involving the same proteins across different dimensionalities⁹,¹⁰.

In this work, we present an approach that closely mirrors physiological conditions, utilizing flexible bilayers and employing fluorescence recovery after photobleaching (FRAP)¹¹ to quantify the interaction constant, K, between proteins whether embedded within membranes or not.

Our investigation leverages the $L_3$ (or sponge) phase, conceptualized as a “melted” cubic phase featuring an isotropic structure¹². This phase comprises a bilayer centered on a minimal (zero mean curvature) surface,

<footnote n="1">¹Laboratoire de Physique de l'École normale superieure, École Normale Supérieure, Université Paris Sciences et Lettres, CNRS, Sorbonne Université, Université Paris Cité, F-75005 Paris, France. ²Department of Infectious Diseases, Avicenne Hospital, AP-HP, Université Sorbonne Paris Nord, Bobigny, France. ³Université Paris Cité, Inserm UMR-S 1266, Institute of Psychiatry and Neuroscience of Paris (IPNP), Paris, France. ⁴Sorbonne Université, CNRS, INSERM, Laboratoire d'Imagerie Biomédicale-LIB, 75006 Paris, France. ⁵Laboratoire CiTOm, Faculté de Santé, Université Paris Cité, CNRS, 75006 Paris, France. ⁶Université Paris Cité, CNRS, Expression Génétique Microbienne, Institut de Biologie Physico-Chimique, Paris, France. ⁷Université Paris Cité, Laboratoire de Biologie Physico-Chimique des Protéines Membranaires CNRS UMR7099, 75005 Paris, France. ⁸Institut de Biologie Physico-Chimique, Fondation Edmond de Rothschild, 75005 Paris, France. ⁹email: vladimir.adrien@aphp.fr; frederic.pincet@ens.fr; urbach@lps.ens.fr</footnote>
dividing space into two interpenetrating solvent labyrinths. Elucidation of this intricate structure derives from diverse scattering data types, encompassing X-rays, neutrons, and light, along with transport properties¹³⁻¹⁵. On a local scale, the L₃ phase's structure resembles that of the lamellar Lα phase¹³. However, on a larger scale, the infinite bilayer separates two interwoven, equivalent, and self-connected solvent domains¹⁶. The appearance of the L₃ phase can be theoretically interpreted as a transition from the ordered cubic arrangement of the membrane to a sponge-like membrane structure, as the regular periodic structure of the cubic phase gets perturbed by bilayer thermal fluctuations, introducing defects that drive the transformation into a sponge-like configuration. Spectra obtained from radiation scattering manifests a well-defined Gaussian peak indicating an average characteristic distance, d<sub>w</sub>¹⁷.

The capacity to compare a two-dimensional system when a protein is membrane-anchored and a three-dimensional situation with the protein in solution stands pivotal in comprehensively determining and predicting their physiological conduct. The three scenarios—both proteins in membranes ("2-d"), one protein in a membrane and the other in solution ("2.5-d"), and both proteins in solution ("3-d")—can be comparatively examined within the same protein pair. We demonstrate the full potential of this approach through two examples: (i) the streptavidin/biotin complex, commonly employed as a reference for robust ligand-receptor pairs, and (ii) an efflux pump involved in a resistance mechanism developed by Gram-negative bacteria, specifically *Pseudomonas aeruginosa*¹⁸⁻²⁰. In the latter case, we utilize two proteins within the three-protein complex forming the principal efflux pump found in these bacteria: MexA and OprM. MexA¹²,²² functions as a membrane fusion protein (MFP) connected to the inner membrane via a lipid anchor, found in the periplasmic space, while OprM²³ represents a trimeric outer membrane channel belonging to the outer membrane factor family (OMF). Subsequently, "OprM" denotes the entire trimeric channel. Detailed high-resolution structures have been elucidated for these²³⁻²⁵. They interact to form a complex with a two-by-two (2, 4, 6 up to 12) MexA to one OprM²⁶,²⁷. More recently, the ternary OprM-MexA-MexB complex was visualized using high-resolution electron microscopy²⁸. Interaction kinetics differ across different geometries, contingent upon each protein's degrees of freedom, and the rates of association and dissociation between each geometry are linked by a characteristic length. This characteristic length provides a quantitative measure of the relative ease of protein binding across various types of dimensionality.

## Results

### Method to measure 2-d association

Monitoring in situ the interactions of two membrane-bound molecules is challenging especially when these interactions occur between opposing bilayers. The method we propose here is based on two key considerations: 1. The diffusion coefficient of species depends on their binding state; 2. L₃ phases allow easy insertion of membrane-bound proteins, maintaining their activity²⁹, and calibration of the intermembrane distance³⁰. Hence, we propose to obtain the equilibrium constant and kinetic rates between two membrane proteins embedded in bilayers by measuring their diffusion coefficients in a L₃ phase. One of the two proteins is fluorescently labeled, and we performed Fluorescence Recovery After Fringe Pattern Photobleaching (FRAPP) experiments (see "Materials and methods" for details).

When the bound and unbound states of fluorescent protein are present in the system, the fluorescence intensity recovery displays a double exponential behavior, as long as any temporal changes of the sample are much slower than the time scale of the experiment:

$$I(t) = I_F \left(1 - e^{-\frac{t}{\tau_F}}\right) + I_B \left(1 - e^{-\frac{t}{\tau_B}}\right). \quad (1)$$

The two diffusion times $\tau_F$ and $\tau_B$ are respectively attributed to the unbound free protein and the bound complex. The surface concentrations of free and bound protein are extracted from the plateau intensities $I_F$ and $I_B$.

We will show below that measuring the diffusion coefficients at various ratios of the two membrane-bound biological objects is sufficient to accurately measure their 2-d dissociation constant, $K_{2d}$, on- and off rates ($k_{on}$ and $k_{off}$ respectively) in trans and in cis.

### 2-d association in trans

#### *Diffusion coefficients of free and bound MexA*

In this section, we model the 2-d association of proteins in two opposite bilayers (i.e. in trans configuration) with the example of OprM and MexA. To measure the 2-d affinity between OprM and MexA, we inserted them inside a L3 phase with a 20 nm intermembrane distance because we previously found that MexA and OprM interact only when they face each other in opposite membranes separated by 20 ± 2 nm²⁶. Since OprM is a large protein complex with transmembrane domains, OprM-bound MexA diffuses much slower than free MexA. Hence, we chose to fluorescently label MexA with FITC. This labeling strategy will ensure that the fluorescence recovery signals can be easily differentiated between free and bound MexA proteins²⁶,³¹. As expected, the recovery signals exhibit a double exponential behavior with two characteristic times for the free and bound states (Fig. 1a and b), that correspond to diffusion coefficients $D_F = 4.5 \pm 0.5 \ \mu m^2 \cdot s^{-1}$ and $D_B = 0.6 \pm 0.1 \ \mu m^2 \cdot s^{-1}$ respectively. $D_F$ is the diffusion coefficient previously measured for MexA alone²⁶. $D_B$ is lower than the coefficient of OprM alone (which we measured at 1.3 ± 0.1 $\mu m^2 \cdot s^{-1}$), probably because bound MexA that is anchored to a bilayer, constraints OprM's mobility.

To obtain the actual amount of each species, the fluorescence intensities must be converted to proportional concentrations. At pH = 8²⁶, bound MexA is found in two types of complexes: one MexA bound to one OprM (A₁M) and two MexA bound to one OprM (A₂M) that contribute to fluorescence intensity of $I_{A₁M}$ and $I_{A₂M}$ respectively. Because we observed a single characteristic time $\tau_B$, our FRAPP measurements done at steady-state (~3–4 h) did not allow us to distinguish the two proteins complexes A₁M and A₂M indicating their diffusion
<figure><img src="image_4.png" /><figcaption>**Figure 1.** Association between proteins (MexA-OprM) embedded in two opposite bilayers (2-d in trans). (a) Typical FRAPP fluorescence recovery curve. It tends to zero since our FRAPP device directly subtracts the intensity value in Eq. (1) to the $I_F + I_B$ plateau intensity. A bi-exponential fit (green curve) fits better the data than a mono-exponential one (red curve) as shown by the residuals in (b), which means that in this case there are two diffusing objects at different mobilities. $I_F$ and $I_B$ are the fluorescence intensities respectively of MexA free and bound to OprM. (c) and (d) Labelled MexA proteins are introduced in a sample containing OprM. Evolution of $I_F$ with the initial molar ratio $r_{AM} = n_{MexA_0}/n_{OprM_0}$ (where $n_{MexA_0}$ and $n_{OprM_0}$ are the input quantities of MexA and OprM respectively). These results are well-fitted by two different segments (---). The ratio between the two slopes gives a dissociation constant $K_{2d} = (8.1 \pm 0.61) 10^{-15} \text{ mol} \cdot \text{dm}^{-2}$. (e) Temporal evolution of $I_B/(I_F + I_B)$ when unlabeled MexA proteins are added in large amount to a L$_3$ phase containing labelled MexA associated with OprM in stoichiometric condition. The two kinds of MexA proteins are competitors for the interaction with OprM. A fit of the temporal evolution (Eq. (S13) in Supplementary Information, section "2-d association in trans") gives a dissociation rate $k_{off} = (1.0 \pm 0.13) 10^{-4} \text{ s}^{-1}$. The deduced association rate is $k_{on,2d} = (1.23 \pm 0.19) 10^{10} \text{ mol}^{-1} \text{ dm}^{-2} \text{ s}^{-1}$. (f) Numerical solution of the evolution of the concentration of the free MexA protein with $r_{AM}$ (Eq. (S2) in Supplementary Information, Sect. 1, with $K_{2d} = (8.1 \pm 0.61) 10^{-15} \text{ mol} \cdot \text{dm}^{-2}$). (g) Numerical solution of the evolution of the concentration of the bound MexA protein, either in the A$_1$M complex (- -) or the A$_2$M complex (---) with $r_{AM}$ (Eq. (S2) in Supplementary Information, Sect. 1, with $K_{2d} = (8.1 \pm 0.61) 10^{-15} \text{ mol} \cdot \text{dm}^{-2}$).</figcaption></figure>

coefficients are similar. This similarity between the two diffusion coefficients was expected since OprM is much larger than MexA and possesses many transmembrane domains. The combined FRAPP of A$_1$M and A$_2$M is represented by $I_B$:

$$I_B = I_{A_1M} + I_{A_2M}. \qquad (2)$$

### Dissociation constant, on- and off-rates

$K_{2d}$ was determined by plotting the variations of $I_F$ with the initial molar ratio $r_{AM} = n_{MexA_0}/n_{OprM_0}$ where $n_{MexA_0}$ and $n_{OprM_0}$ are the input quantities of MexA and OprM respectively (corresponding to concentrations of 0.2 µM and 2 µM). $I_F$ exhibits a linear behavior before and after $r_{AM} = 2$ (see Fig. 1c and d and Supplementary Information, Sect. 1 for a detailed explanation). The ratio between the two slopes gives $K_{2d} = 8.1 10^{-15} \pm 0.61 10^{-15} \text{ mol} \cdot \text{dm}^{-2}$.

We then implemented the following protocol to measure the off-rate $k_{off}$. OprM and labeled MexA were mixed in the same L$_3$ sample in stoichiometric conditions (2 MexA for 1 OprM at 3.2 and 1.6 µM respectively). We prepared the same solution with unlabeled MexA proteins at a concentration 100 times higher. Equal volumes of both solutions were gently mixed. Because of the excess of unlabeled MexA, bound labeled MexA were then replaced by unlabeled one. The kinetics of this replacement process is limited by the unbinding of labeled MexA
and thus directly linked to the off-rate of MexA. Recovery curves obtained for different waiting times after mixing directly provided a quantitative measure of this replacement. The variations of $I_B/(I_F + I_B)$ are displayed in Fig. 1e. This ratio first seems to be constant and then decreases with time.

A numerical adjustment of the temporal evolution of the ratio $I_B/(I_F + I_B)$ (Fig. 1e) gives the off-rate (see Supplementary Information, section "2-d association in trans"): $k_{off} = (1.0 \pm 0.13) \ 10^{-4} \text{ s}^{-1}$. The time resolution of our experiment of the order of 60 s makes it possible to measure an off-rate below $10^{-2} \text{ s}^{-1}$ which is comparable with standard techniques like Surface Plasmon Resonance³².

The corresponding on-rate $k_{on,2d} = k_{off}/K_{2d}$ is ~ (1.2 ± 0.19) $10^{10} \text{ mol}^{-1} \text{ dm}^2 \text{ s}^{-1}$. This is consistent with the fact that with a surface concentration [MexA] ~ 1 pmol dm$^{-2}$ (see Supplementary Information, section "3-d association") the association time $1/(k_{on,2d}[\text{MexA}])$ is ~ 80 s. Indeed, our association experiments showed that equilibrium is reached in a time smaller than a few minutes.

## 2-d association in cis

To model 2-d affinities between two proteins embedded in the same membrane (cis configuration) we focused on the interactions between a biotinylated transmembrane peptide $BL_{12}$ noted B, and labeled streptavidin S ³³,³⁴. The separation between bilayers is 12 nm which is much larger than the dimension of S thus preventing any trans interactions: streptavidin can only be linked to peptides anchored in the same bilayer, as previously demonstrated²⁶. S possesses four B binding pockets but can only be bound to a maximum of two B in cis-interaction³⁵.

In time, the first reaction is the binding of a free soluble S to a membrane-bound B forming a $B_1S$ complex with an on-rate $k_{on,2.5d}$. We call this type of reaction with a soluble protein binding a membrane-anchored "2.5-d reactions". This will be discussed in the next section. The second reaction is the association between two peptides diffusing in the same membrane, a $B_1S$ to a free B forming a $B_2S$ complex with an on-rate $k_{on,2d}$. The corresponding dissociation reactions are not considered, as the lifetimes $\tau$ of the complexes between S and B ($\tau \approx 10^7$ s)³⁶ are much longer than the timescale of the experiment (~3–4 h). We assume $k_{off} \approx 0$, thus the equilibrium is reached when $[B] = 0$.

FRAPP measurements on FITC-labelled S allow distinguishing between the free S, the complexes $B_1S$ and $B_2S$ as their diffusion coefficients are $D_{0S} = 50 \pm 2.4 \ \mu\text{m}^2 \text{s}^{-1}$, $D_{1S} = 3.2 \pm 0.2 \ \mu\text{m}^2 \text{s}^{-1}$ and $D_{2S} = 1.6 \pm 0.1 \ \mu\text{m}^2 \text{s}^{-1}$ respectively. The corresponding plateau intensities from the recovery signal are called $I_{0S}$, $I_{1S}$ and $I_{2S}$. We checked that $[B_1S]$ and $[B_2S]$ are proportional to $I_{1S}$ and $I_{2S}$ (see Supplementary Information, Sect. 4).

We introduced a constant concentration of streptavidin $S_0 = 9.7 \ 10^{-7} \text{ M}$ and varied the concentration of B. Figure 2a shows the evolution of $I_{2S}/I_{1S}$ versus the initial molar ratio $r_{BS} = n_{B_0}/n_{S_0}$ where $n_{B_0}$ and $n_{S_0}$ are the initial quantities of B and S respectively. This ratio is increased by varying the peptide quantity. At small $r_{BS}$ (large excess of S), the concentration of S is almost constant and equal to the initial concentration $S_0$, and we can consider that its bound fraction is negligible. We thus predict (see Supplementary Information, Sect. 5) that $I_{2S}/I_{1S}$ should vary linearly with a slope proportional to $k_{on,2d}/k_{on,2.5d}$. The data are indeed linear (see Fig. 2b) and lead to $k_{on,2.5d}/k_{on,2d} = 6.4 \pm 0.5 \text{ nm}$. Using the known value of $k_{on,2.5d}$ (~$10^6-1.3 \cdot 10^7 \text{ M}^{-1} \text{s}^{-1}$)³⁷,³⁸, we find that $k_{on,2d} \sim 1-2.10^{14} \text{ mol}^{-1} \text{ dm}^2 \text{ s}^{-1}$. Finally, we plotted the predicted variations (see Supplementary Information, Sect. 6) of $I_{2S}/I_{1S}$ over a wider range of $r_{BS}$ using $k_{on,2.5d}/k_{on,2d}$ measured for small $r_{BS}$. The resulting curves nicely fit the experimental data, confirming the validity of our approach (Fig. 2).

<figure><img src="image_5.png" /><figcaption>**Figure 2.** Association between proteins (Streptavidin–biotin) anchored in the same bilayer (2-d in cis). $I_{1S}$ and $I_{2S}$ are the fluorescence intensities respectively of an S bound to a membrane-anchored B forming a $B_1S$ complex and a $B_1S$ to a second membrane-anchored B forming a $B_2S$ complex. (a) Results obtained for the variation of the ratio between the intensities $I_{2S}/I_{1S}$ for different initial molar ratios $r_{BS} = n_{B_0}/n_{S_0}$ (where $n_{B_0}$ and $n_{S_0}$ are the initial quantities of B and S respectively). Results are compared over a wider range of $r_{BS}$ to numerical models from kinetic equations (see Eq. (S23) in Supplementary Information, Sect. 5) performed for $k_{on,2.5d} = 10^6 \text{ M}^{-1} \text{s}^{-1}$ and $k_{on,2d} = 2.5 \cdot 10^{13} \text{ mol}^{-1} \text{ dm}^2 \text{ s}^{-1}$ (- -) Error bars are not visible when they are lower than the size of the dot. (b) For small $r_{BS}$ values, $I_{2S}/I_{1S}$ varies linearly with $r_{BS}$ with a slope proportional to $k_{on,2.5d}/k_{on,2d}$ and a straight line adjustment (- -) gives $k_{on,2.5d}/k_{on,2d} = 6.4 \pm 0.5 \text{ nm}$.</figcaption></figure>
## 2.5-d association

Here we study the interactions between a membrane bound protein and a partner freely diffusing in the inter-membrane space. As mentioned in the previous section, this kind of “2.5-d” association for the S/B pair has already been measured with different techniques³⁷,³⁸. Hence, we will focus on OprM and MexA using an FITC-labeled soluble mutant of MexA (mMexA) which has a deleted unique N-terminal cysteine preventing anchor-age to the membrane. mMexA is solubilized in the intermembrane space of the L₃ phase³⁹ in which an OprM is embedded. In this situation, MexA has more degrees of freedom in comparison to when it is embedded in the membrane.

In a first experiment, we tested mMexA diffusion alone (at 0.2 µM) in the L₃ phase and measured a single diffusion coefficient, D = 20 ± 1 µm².s⁻¹ which is consistent with the diffusion of a soluble element in a L₃ phase⁴⁰. In another experiment, a large excess of OprM protein was added to the L₃ phase at 2 µM with an initial molar ratio r<sub>mAM</sub> = n<sub>mMexA0</sub>/n<sub>OprM0</sub> = 0.1, where n<sub>mMexA0</sub> and n<sub>OprM0</sub> are the input concentrations of mMexA and OprM). As in 2-d experiment, the recovery signals exhibit a double exponential behavior (Eq. 1).

The two diffusion times τ<sub>F</sub> and τ<sub>B</sub> are related to diffusion coefficient values of D<sub>F</sub> = 20 µm².s⁻¹ and D<sub>B</sub> = 1.4 µm².s⁻¹. D<sub>F</sub> is the diffusion coefficient of mMexA diffusing “freely” in the intermembrane space. D<sub>B</sub> corresponds exactly to the diffusion coefficient of OprM alone and we associate this value to mMexA bounded to OprM. Since the OprM protein is in large excess (r<sub>mAM</sub> = 0.1, we assume here that only one mMexA protein can bind an OprM. This assumption is supported by the fact that in 2-d geometry, when r<sub>AM</sub> < 0.5, the A₁M complex was dominant (Fig. 1c).

The measured intensities I<sub>mF</sub> and I<sub>mB</sub> corresponding to each diffusion time are proportional to the number of the free and bound mMexA. We obtained FRAPP signals for different waiting times after the initial mixing of the components. The intensities I<sub>mF</sub> and I<sub>mB</sub> are changing with time: I<sub>mF</sub> decreases while I<sub>mB</sub> increases (Fig. 3a and b) attesting the formation of the mA₁M complex.

The kinetics of the reaction can be quantitatively described (see Supplementary Information, Sect. 7). The on-rate, k<sub>on,2.5d</sub>, and off-rate, k<sub>off</sub>, can be obtained by a simultaneous fit of I<sub>mF</sub>/I<sub>mB</sub> and I<sub>mF</sub> + I<sub>mB</sub> over time. The deduced association and dissociation rates are k<sub>on,2.5d</sub> = 131 ± 17 M⁻¹.s⁻¹ and k<sub>off</sub> = (0.6 ± 0.2) s⁻⁴. The small k<sub>on,2.5d</sub> value, compared to common receptor-ligand associations (on-rates of the order of 10⁵–10⁷ M⁻¹.s⁻¹)⁴¹, shows that the mMexA-OprM association in the 2.5-d geometry has a low probability to occur. Still, the value of k<sub>off</sub> corresponds to common receptor-ligand associations⁴¹ and gives a lifetime of the bond of about 4.6 h indicating the mMexA-OprM complex is highly stable with a dissociation energy barrier of approximately 30 k<sub>B</sub>T⁴². Furthermore, this k<sub>off</sub> value is compatible with the one found in the 2-d geometry and shows that the off-rate does not depend on the geometry. Finally, we can deduce the dissociation constant: K<sub>2.5d</sub> = k<sub>off</sub>/k<sub>on,2.5d</sub> = (4.6 ± 1.5)0.10⁻⁷ M. It corresponds to a relatively low affinity for membrane proteins associations. This range is comparable to the ones obtained for interactions between acid sialic and membrane receptors⁴³, dimerization of the glycophorinA⁴⁴ or various enzyme and substrate interactions⁴¹.

## 3-d association

We used the standard micellar approach to study the interaction between mMexA and OprM in the same saline buffer used to prepare the L₃ phase. OprM was solubilized in β-OG at 0.9% (w/vol). The concentration of OprM was kept constant (0.8 µM) while the mMexA rate increased (r<sub>mAM</sub> from 0 to 15). After 24 h, for all the values of r<sub>mAM</sub>, we observed single exponential fluorescence recovery curves, corresponding to diffusion coefficients, D, equal to the ones measured when mMexA is alone in solution at the same concentrations (Fig. 4). According to Stokes–Einstein equation, the order of magnitude of the diffusion coefficients correspond to a radius of 2.3 ± 0.1 nm for mMexA which is consistent with its crystal structure²¹. If MexA were linked to OprM, this would

<figure><img src="image_6.png" /><figcaption>**Figure 3.** Association between proteins (mMexA-OprM) when MexA is soluble and OprM is embedded in the bilayer (2.5-d). (a) Temporal evolution of the intensity I<sub>mF</sub> of free mMexA. Results are fitted by an exponential law (Eq. S42) in Supplementary Information, Sect. 7). It provides the characteristic time τ of 1150 ± 119 s. (b) Evolution of the intensity I<sub>mB</sub> of mMexA bound to OprM with time. Results are fitted by an exponential law (Eq. S42). It provides the characteristic time τ of 973 ± 151 s. These two results are compatible. The mean time τ is deduced: τ = 1061 ± 136 s.</figcaption></figure>
<figure><img src="image_7.png" /><figcaption>**Figure 4.** Association between proteins (mMexA-OprM) solubilized in solution (3-d configuration). Variation of diffusion coefficients *D* with *r*<sub>mAM</sub> = *n*<sub>mMexA0</sub>/*n*<sub>OprM0</sub> (where *n*<sub>mMexA0</sub> and *n*<sub>OprM0</sub> are the input quantities of mMexA and OprM respectively) of FITC-labeled mMexA in solution in the presence of OprM at a concentration of 0.8 µM after 24 h of mixing both proteins. The high values of the diffusion coefficients indicate that mMexA does not interact with OprM. Their decrease with concentration is attributed to possible dimerization or limited aggregation of mMexA.</figcaption></figure>

slow down the diffusion of MexA. We would then observe a double exponential corresponding to two diffusion coefficients, the free and bound mMexA. One of the exponential due to the free mMexA would represent a diffusion coefficient of *D* equal to the diffusion coefficients of mMexA alone in solution at the same concentrations. Because of the large size of OprM compared to the micelle radius, the second exponential, due to bound mMexA, would represent a diffusion coefficient similar to that of OprM alone at the same concentration, i.e. *D* = 32 ± 0.4 µm2.s⁻¹, which corresponds to a Stokes radius of 6.7 nm consistent with the crystal structure of OprM²³,⁴⁵. Hence, our results suggest that mMexA does not interact with OprM in 3-d geometry. This was confirmed by blue native polyacrylamide gel electrophoresis²⁷. The value of *K*₃d is therefore must be much higher than *K*₂.₅d, indicating a lower affinity in three dimensions.

Discussion

2-d association in trans

We presented in this article a simple and original approach to measure the affinity between two membrane proteins in the *trans* configuration. Other methods can be mechanical (e.g. micromanipulation assays between two cells⁹,¹⁰. Our approach allows us to measure 2-d affinities up to 10⁻¹⁴ mol.dm⁻². The tunable inter-bilayer distance from 5 to 30 nm of the L₃ phase makes it possible to study other membrane protein *trans* interactions in gram-negative bacteria (both membranes being separated by 20 nm) or mitochondria (22 nm), trans-synaptic complexes (the height of a chemical synaptic cleft being of 10–30 nm)⁴⁶⁻⁴⁹, lipid transfer proteins and other complexes that connect the endoplasmic reticulum to plasma membrane (again with a gap typically within 10 to 30 nm)⁵⁰,⁵¹ or the two membranes of the autophagosome (10–30 nm also)⁵².

We solved the equilibrium (Eq. (S1) in Supplementary Information) with $K_{2d} = (8.1 \pm 0.61) \times 10^{-15} \text{ mol dm}^{-2}$ (Fig. 1f and g). For $r_{AM} > 2$, only the $A_2M$ complex is present; again, this confirms our previous assumption: we considered $[A_1M]$ to be negligible compared to $[A_2M]$.

Furthermore, Fig. 1g explains why no significant break in the slope of $I_F$ was observed in Fig. 1c when $r_{AM} = 1$. It might have been supposed that the slope when $r_{AM} < 1$ would be the same as when $r_{AM} > 2$, if MexA proteins would only form $A_1M$ complexes. This is not the case because when $r_{AM} < 1$, $A_2M$ cannot be neglected. Probable quenching effects even at low $r_{AM}$ explain why the slope is lower also for $r_{AM} < 1$ than for $r_{AM} > 2$. Our results also allow us to predict that all $A_2M$ complexes are assembled in the bacteria. Narita et al. count 2500 MexA and 1200 OprM per bacteria. Modeling a bacteria as a sphere of radius 1 µm, the surface concentration in MexA and OprM is ~10⁻¹² mol.dm⁻²⁵³. The 2-d dissociation constant measured here, $K_{2d} = (8.1 \pm 0.61) \times 10^{-15} \text{ mol dm}^{-2}$, indicate that all MexA and OprM will associate in the bacteria if all OprM proteins are accessible.

Significance of the characteristic length linking 2-d to 2.5-d Association

The ratio between the “2.5-d” and the 2-d association rates provides a characteristic length $\Delta = k_{on,2.5d}/k_{on,2d}$. It reflects how much the binding of both proteins to membranes facilitate their association: the smaller $\Delta$, the most favorable the 2-d interactions compared to the 2.5-d interactions. More precisely, in 2.5-d, one of the proteins freely diffuses in the bulk while in 2-d, it remains anchored to the membrane. Hence, the apparent volume concentration of the protein in the 2-d geometry is about: $[P] = \{P\}/\lambda$ where $\{P\}$ is the surface concentration (in mol.dm⁻²) and $\lambda$ is the typical distance between the anchoring point and the binding site, which, in general, is commensurate with the protein size. The 2-d on-rate deduced from this apparent volume concentration and the 2.5-d on-rate would then be: $k_{on,2dapparent} = k_{on,2.5d}/\lambda$. Hence, if $\Delta < \lambda$, the pair will more easily associate in 2-d while if $\Delta > \lambda$ the two partners will better bind in 2.5-d (Fig. 5). For the S/B interactions, $\Delta = 6.4 \pm 0.5$ nm and $\lambda$ is the distance between the two binding pockets, i.e. $\lambda \sim 2.5$ nm⁵⁴. Hence, for the S/B pair, 2-d and 2.5-d are relatively equivalent probably because the bound protein can almost freely rotate when bound to a single B.

The case of the interactions between OprM and MexA is very different. The typical dimension of MexA is $\lambda \sim 3.5$ nm. Our measurements show that for this pair, $\Delta = k_{on,2.5d}/k_{on,2d} = 1.1 \pm 0.18$ nm. Hence, the 2-d association
<figure><img src="image_8.png" /><figcaption>**Figure 5.** Graphical representation of different geometries of protein interaction with $\Delta/\lambda$. The ratio > 1, it favors 2.5-d association, whereas the ratio < 1, favors 2-d interaction.</figcaption></figure>

can be considered about 3 times faster than the 2.5-d association. This difference is key for the association of MexA with OprM because the 2.5-d on-rate, $k_{on,2.5d} = 131 \pm 17$ M⁻¹·s⁻¹ is very small compared to the diffusion-limited collision rate, ~ $10^9$ M⁻¹·s⁻¹, obtained from the classical Smoluchowski expression⁵⁵, $k_{on} = 4\pi DR$ where D is the relative translational diffusion constant and R is the sum of the radii of both diffusing objects.

Having both proteins anchored in opposing membranes significantly accelerates bond formation. In addition, the intermembrane distance is critical because we previously showed that OprM and MexA are unable to bind if the membranes are less than 18 nm or more than 22 nm apart²⁶, meaning that, for these ranges of intermembrane separations, $k_{on,2d} = 0$. To summarize, studying 2-d *trans* interactions can be useful to control the assembly of protein complexes. Indeed, protein orientation plays a key role for interactions of membrane proteins, as already observed⁴. Adjusting intermembrane distances allows facilitating the formation of specific complexes while hindering others.

## 2.5-d to 3-d association

The dissociation constant between mMexA and OprM in 2.5-d being $K_{2.5d} = (4.6 \pm 1.5)0.10^{-7}$ M, if both proteins had the same affinity in the 3-d configuration, we should expect them to significantly bind to each other. Indeed, like for the 2-d geometry, at low $r_{mAM}$, OprM is in large excess, and we can consider that only a single protein could bind to OprM. If we now suppose that the equilibrium constant $K_{3d}$ is equal to $K_{2.5d}$ and of the order of $4.6 \times 10^{-7}$ M, we can calculate the ratio $[mMexA]/[A_1M] = K_{3d}/[\text{OprM}]_0 = 0.46/0.8 = 0.58$. It means that approximately 35% of labelled mMexA would be free and 65% would be bound to OprM. We should thus see a double exponential recovery curve when performing FRAPP experiments. Since we only observed a single exponential recovery curve, $K_{3d}$ must be larger than $K_{2.5d}$, suggesting that it is much more difficult for MexA to bind an OprM that is not membrane-anchored.

To confirm our results, we performed the same experiment with native MexA. It diffuses slower in solution in the presence of OprM than alone (Fig. S7 in Supplementary Information) probably because both proteins gather within detergent micelles. This difference may also come from the fact that native MexA has less degrees of freedom in solution because it is self-rotating along with detergent covering its hydrophobic part, and is thus slowed down in its rotation, thus able to interact with OprM.

Focusing now on the interaction between S and biotin in the 3-d geometry, $K_{3d}$ was measured three decades ago and found to be in the pM range, $2.5 \times 10^{-13}$ M⁵⁶. More recently $K_{2.5d}$ was accurately measured using nanowires coated with biotin and found to be slightly lower, $5.6 \times 10^{-14}$ M⁵⁷. Even though the geometry and freedom of biotin may not be exactly the same as on a membrane, this difference between $K_{3d}$ and $K_{2.5d}$ suggests that, as for OprM and MexA, bond formation is facilitated by placing one of the partners on a surface with the correct orientation.

In this article we provided a new method to systematically compare the kinetic parameters of protein association in volume and on membranes. We presented a single parameter involving the on-rates and the distance, $\lambda$, between the binding and anchoring points of the proteins that quantitatively captures which geometry, 2.5-d or 2-d, is more favorable than the other. This parameter, $k_{on,2.5d}/(k_{on,2d}\lambda)$, globally encapsulates the various degrees of freedom involved in protein interactions including protein orientation that depends on the anchorage to the membrane, fixing them like a keyhole to a door. The orientation of the keyhole makes it easier or more difficult for the key to interact compared to the situation where the keyhole would be moving and self-rotating. We also confirmed the intuitive fact that the off-rates $k_{off}$ do not depend on the geometry of protein interactions.

We demonstrated that time resolved FRAPP experiments in a L₃ phase give precise values for dynamic rates of these associations between soluble and membrane proteins. The time resolution of our technique allows to measure dissociation rates comparable with range obtained by standard techniques⁵⁸. Our approach can be
extended to other techniques such as Single Particle Tracking or Fluorescence Correlation Spectroscopy measurements instead of FRAPP.

## Materials and methods
### Proteins

Fluorescein IsoThioCyanate (FITC)-labeled streptavidin was purchased from Intechim and used as received. The twelve-leucine α-helix transmembrane peptide $L_{12}$ whose sequence is AKK-L$_{12}$-GKK was synthesized and biotinylated ($BL_{12}$) in the Department of Biochemistry and Molecular Genetics (University of Colorado, Denver).

MexA was expressed and purified at 8 mg/mL according to Trépout et al.⁵⁹ in its mature form and its mutant soluble form (with the N-terminal cysteine deleted)⁶⁰. Throughout the manuscript, MexA refers to the palmitoylated version of the protein, that is anchored to the membrane, and mMexA refers to the non-palmitoylated version of the protein.

OprM was expressed and purified at 2 mg/mL as previously described²⁴,⁶¹.

Depending on the experiments, OprM and MexA could be labeled with FITC (Molecular Probes) following the FluoReporter™ FITC Labeling kit protocol. All protein samples were solubilized in a 50 mM phosphate buffer, pH = 8, containing 100 mM NaCl, 5% (v/v) glycerol and n-octyl-β-D-glucopyranoside (β-OG, Sigma Aldrich) at 0.9% (w/vol).

### L$_{3}$ phase

To prepare the $L_{3}$ sponge phase²⁹,⁶²,⁶³, we mixed a non-ionic surfactant, pentaethylene glycol monododecyl ether ($C_{12}E_{5}$, Sigma Aldrich), β-OG, 5% (v/v) glycerol, and NaCl 100 mM and 50 mM phosphate buffer at pH = 8. The molar ratio β-OG:$C_{12}E_{5}$ was kept constant at 1:7.6. In this phase, bilayers are randomly connected but the membrane volume fraction $φ = (V_{β-OG} + V_{C_{12}E_{5}})/V_{solution}$ corresponds to a local intermembrane distance $d_{w}$. We tuned this fraction to have $d_{w} = 20$ nm¹⁷ for experiments involving OprM and MexA (since it is the distance that separates in vivo both Pseudomonas aeruginosa membranes), or $d_{w} = 12$ nm for experiments with streptavidin and biotinylated peptides, which corresponded to membrane volume fractions $φ$ of 0.05 and 0.1 respectively. All samples were of 10 µL. The phase is isotropic and stable at room temperature for several weeks. Proteins were added at relatively low concentrations (0.5 to 4 µM) to the surfactant-buffer solution and the sample was vortexed for a few seconds before letting it rest at room temperature for a few minutes prior to proceeding with diffusion measurements. The samples were kept for several weeks at 4 °C and remained stable under these conditions.

### Fluorescence recovery after fringe pattern photobleaching (FRAPP)

The sample was injected into a capillary tube of a 200 µm thickness (VitroCom, Mountain Lakes, New Jersey) which was sealed with wax in order to prevent evaporation. The diffusion coefficient was obtained by performing FRAPP on the sample¹¹,⁶⁴: the laser was focused on a dot of approximately 250 µm of diameter, to insure that the entire thickness of the sample is bleached in order to measure the lateral fluorescence recovery only. The fringe pattern was tuned with various interfringe distances ranging from 10 to 50 µm. The fact that the diffusion is Brownian was verified by using the equation:

$$D = \frac{i^2}{4\pi^2\tau}, \qquad (3)$$

where i is the interfringe distance and τ is the recovery time. The fringe pattern has the asset of having a simple geometry: the fluorescence recovery curves were thus easy to fit, τ being obtained by fitting them with a simple exponential if there was one diffusing regime, or a double exponential if the object (lipid, peptide or protein) was diffusing at two different speeds, or if there were two objects diffusing differently. FRAPP measurements on the $L_{3}$ phase are accurate: the phase being isotropic and formed on a large volume, bleaching experiments are automatized in order to sum up at least 10 times the fluorescence recovery curves and reduce the noise. The $L_{3}$ phase is volumetric, so there is no problem of fluorescence loss or acquisition bleaching. In total, we were able to measure the diffusion coefficient of an object in the sponge phase with an accuracy of 2 to 5%.

### Data availability

The datasets generated and analyzed during the current study are available from the corresponding author on reasonable request.

Received: 2 April 2023; Accepted: 26 December 2023

Published online: 09 January 2024

### References

1. Adam, G. & Delbruck, M. Reduction of dimensionality in biological diffusion processes. In *Structural Chemistry and Molecular Biology* (eds Rich, A. & Davidson, N.) 198–215 (W H. Freeman and Co., 1968).

2. Axelrod, D. & Wang, M. D. Reduction-of-dimensionality kinetics at reaction-limited cell surface receptors. *Biophys. J.* **66**, 588–600 (1994).

3. Baudry, J. et al. Acceleration of the recognition rate between grafted ligands and receptors with magnetic forces. *Proc. Natl. Acad. Sci.* **103**, 16076–16078 (2006).

4. Gavutis, M., Jaks, E., Lamken, P. & Piehler, J. Determination of the two-dimensional interaction rate constants of a cytokine receptor complex. *Biophys. J.* **90**, 3345–3355 (2006).

5. Gavutis, M., Lata, S. & Piehler, J. Probing 2-dimensional protein-protein interactions on model membranes. *Nat. Protoc.* **1**, 2091–2103 (2006).
6. MacKenzie, K. R., Prestegard, J. H. & Engelman, D. M. A transmembrane helix dimer: Structure and implications. *Science* **276**, 131–133 (1997).

7. Fisher, L. E., Engelman, D. M. & Sturgis, J. N. Detergents modulate dimerization, but not helicity, of the glycophorin A transmembrane domain. *J. Mol. Biol.* **293**, 639–651 (1999).

8. Miller, S. E., Collins, B. M., McCoy, A. J., Robinson, M. S. & Owen, D. J. A SNARE-adaptor interaction is a new mode of cargo recognition in clathrin-coated vesicles. *Nature* **450**, 570–574 (2007).

9. Huang, J. et al. Quantifying the effects of molecular orientation and length on two-dimensional receptor-ligand binding kinetics \*.* *J. Biol. Chem.* **279**, 44915–44923 (2004).

10. Dustin, M. L., Bromley, S. K., Davis, M. M. & Zhu, C. Identification of self through two-dimensional chemistry and synapses. *Annu. Rev. Cell Dev. Biol.* **17**, 133–157 (2001).

11. Davoust, J., Devaux, P. F. & Legerl, L. Fringe pattern photobleaching, a new method for the measurement of transport coefficients of biological macromolecules. *EMBO J.* **1**, 1233–1238 (1982).

12. Porte, G. Isotropic phases of bilayers. *Curr. Opin. Colloid Interface Sci.* **1**, 345–349 (1996).

13. Maldonado, A. et al. Confined diffusion in a sponge phase. *J. Phys. Chem. B* **108**, 2893–2897 (2004).

14. Porte, G., Marignan, J., Bassereau, P. & May, R. Shape transformations of the aggregates in dilute surfactant solutions: A small-angle neutron scattering study. *J. Phys. Fr.* **49**, 511–519 (1988).

15. Gazeau, D., Bellocq, A. M., Roux, D. & Zemb, T. Experimental evidence for random surface structures in dilute surfactant solutions. *Europhys. Lett.* **9**, 447 (1989).

16. Porte, G., Appell, J., Bassereau, P. & Marignan, J. La to L3: A topology driven transition in phases of infinite fluid membranes. *J. Phys. Fr.* **50**, 1335–1347 (1989).

17. Adrien, V. et al. Characterization of a biomimetic mesophase composed of nonionic surfactants and an aqueous solvent. *Langmuir* **32**, 10268–10275 (2016).

18. Andersen, C., Hughes, C. & Koronakis, V. Chunnel vision. Export and efflux through bacterial channel-tunnels. *EMBO Rep.* **1**, 313–318 (2000).

19. McKeegan, K. S., Borges-Walmsley, M. I. & Walmsley, A. R. Microbial and viral drug resistance mechanisms. *Trends Microbiol.* **10**, S8-14 (2002).

20. Poole, K. Multidrug resistance in gram-negative bacteria. *Curr. Opin. Microbiol.* **4**, 500–508 (2001).

21. Akama, H. et al. Crystal structure of the membrane fusion protein, MexA, of the multidrug transporter in *Pseudomonas aeruginosa*. *J. Biol. Chem.* **279**, 25939–25942 (2004).

22. Higgins, M. K., Bokma, E., Koronakis, E., Hughes, C. & Koronakis, V. Structure of the periplasmic component of a bacterial drug efflux pump. *Proc. Natl. Acad. Sci.* **101**, 9994–9999 (2004).

23. Akama, H. et al. Crystal structure of the drug discharge outer membrane protein, OprM, of *Pseudomonas aeruginosa*: Dual modes of membrane anchoring and occluded cavity end. *J. Biol. Chem.* **279**, 52816–52819 (2004).

24. Phan, G. et al. Structural and dynamical insights into the opening mechanism of *P. aeruginosa* OprM channel. *Structure* **18**, 507–17 (2010).

25. Symmons, M. F., Bokma, E., Koronakis, E., Hughes, C. & Koronakis, V. The assembled structure of a complete tripartite bacterial multidrug efflux pump. *Proc. Natl. Acad. Sci.* **106**, 7173–7178 (2009).

26. Reffay, M. et al. Tracking membrane protein association in model membranes. *PLoS One* **4**, e5035 (2009).

27. Ferrandez, Y. et al. Stoichiometry of the MexA-OprM binding, as investigated by blue native gel electrophoresis. *Electrophoresis* **33**, 1282–1287 (2012).

28. Glavier, M. et al. Antibiotic export by MexB multidrug efflux transporter is allosterically controlled by a MexA-OprM chaperone-like complex. *Nat. Commun.* **11**, 1–11 (2020).

29. Rayan, G. et al. Surfactant bilayers maintain transmembrane protein activity. *Biophys. J.* **107**, 1129–1135 (2014).

30. Safinya, C. R., Sirota, E. B., Roux, D. & Smith, G. S. Universality in interacting membranes: The effect of cosurfactants on the interfacial rigidity. *Phys. Rev. Lett.* **62**, 1134–1137 (1989).

31. Gambin, Y. et al. Lateral mobility of proteins in liquid membranes revisited. *Proc. Natl. Acad. Sci.* **103**, 2098–2102 (2006).

32. Beeg, M. et al. Surface plasmon resonance unveils important pitfalls of enzyme-linked immunoassay for the detection of anti-infl iximab antibodies in patients’ sera. *Sci. Rep.* **11**, 14976 (2021).

33. Hendrickson, W. A. et al. Crystal structure of core streptavidin determined from multiwavelength anomalous diffraction of syn-chrotron radiation. *Proc. Natl. Acad. Sci.* **86**, 2190–2194 (1989).

34. Weber, P. C.,ohlendorf, D. H., Wendoloski, J. J. & Salemme, F. R. Structural origins of high-affinity biotin binding to streptavidin. *Science* **243**, 85–88 (1989).

35. Fairhead, M., Krndija, D., Lowe, E. D. & Howarth, M. Plug-and-play pairing via defined divalent streptavidins. *J. Mol. Biol.* **426**, 199–214 (2014).

36. Pincet, F. & Husson, J. The solution to the streptavidin-biotin paradox: The influence of history on the strength of single molecular bonds. *Biophys. J.* **89**, 4374–4381 (2005).

37. Buranda, T. et al. Ligand receptor dynamics at streptavidin-coated particle surfaces: A flow cytometric and spectrofluorimetric study. *J. Phys. Chem. B* **103**, 3399–3410 (1999).

38. Qureshi, M. H., Yeung, J. C., Wu, S. C. & Wong, S. L. Development and characterization of a series of soluble tetrameric and monomeric streptavidin muteins with differential biotin binding affinities. *J. Biol. Chem.* **276**, 46422–46428 (2001).

39. Cates, M. E. & Roux, D. Random bilayer phases of dilute surfactant solutions. *J. Phys. Condens. Matter* **2**, SA339 (1990).

40. Anderson, D. M. & Wennerstroem, H. Self-diffusion in bicontinuous cubic phases, L3 phases, and microemulsions. *J. Phys. Chem.* **94**, 8683–8694 (1990).

41. Dukhovich, F. S., Gorbatova, E. N., Darkhovskii, M. B. & Kurochkin, V. K. Relationship between the dissociation constant and the lifetime for complexes of biologically active substances with receptors and enzymes. *Pharm. Chem. J.* **36**, 248–254 (2002).

42. Evans, E. Energy landscapes of biomolecular adhesion and receptor anchoring at interfaces explored with dynamic force spectroscopy. *Faraday Discuss.* https://doi.org/10.1039/a809884k (1998).

43. Moore, J. et al. Recognition of saccharides by the OpcA, OpaD, and OpaB outer membrane proteins from *Neisseria meningitidis*. *J. Biol. Chem.* **280**, 31489–31497 (2005).

44. Fisher, L. E., Engelman, D. M. & Sturgis, J. N. Effect of detergents on the association of the glycophorin A transmembrane helix. *Biophys. J.* **85**, 3097–3105 (2003).

45. Monlezun, L. et al. New OprM structure highlighting the nature of the N-terminal anchor. *Front. Microbiol.* https://doi.org/10.3389/fmicb.2015.00667 (2015).

46. Biederer, T., Kaeser, P. S. & Blanpied, T. A. Transcellular nanoalignment of synaptic function. *Neuron* **96**, 680–696 (2017).

47. Elegheert, J. et al. Structural basis for integration of GluD receptors within synaptic organizer complexes. *Science* **353**, 295–300 (2016).

48. Tang, A. H. et al. A trans-synaptic nanocolumn aligns neurotransmitter release to receptors. *Nature* **536**, 210–214 (2016).

49. Savtchenko, L. P. & Rusakov, D. A. The optimal height of the synaptic cleft. *Proc. Natl. Acad. Sci.* **104**, 1823–1828 (2007).

50. Li, C. et al. Endoplasmic reticulum-plasma membrane contact sites: Regulators, mechanisms, and physiological functions. *Front. Cell Dev. Biol.* **9**, 627700 (2021).
51. Wong, L. H., Gatta, A. T. & Levine, T. P. Lipid transfer proteins: The lipid commute via shuttles, bridges and tubes. *Nat. Rev. Mol. Cell Biol.* **20**, 85–101 (2019).

52. Nguyen, N., Shteyn, V. & Melia, T. J. Sensing membrane curvature in macroautophagy. *J. Mol. Biol.* **429**, 457–472 (2017).

53. Narita, S., Eda, S., Yoshihara, E. & Nakae, T. Linkage of the efflux-pump expression level with substrate extrusion rate in the MexAB-OprM efflux pump of *Pseudomonas aeruginosa*. *Biochem. Biophys. Res. Commun.* **308**, 922–926 (2003).

54. Le Trong, I. et al. Streptavidin and its biotin complex at atomic resolution. *Acta Crystallogr. D Biol. Crystalogr.* **67**, 813–821 (2011).

55. Smoluchowski, M. V. Mathematical theory of the kinetics of the coagulation of colloidal solutions. *Z. Phys. Chem.* **92**, 129–168 (1917).

56. Weber, P. C., Wendoloski, J. J., Pantoliano, M. W. & Salemme, F. R. Crystallographic and thermodynamic comparison of natural and synthetic ligands bound to streptavidin. *J. Am. Chem. Soc.* **114**, 3197–3200 (1992).

57. Duan, X. et al. Quantification of the affinities and kinetics of protein interactions using silicon nanowire biosensors. *Nat. Nanotechnol.* **7**, 401–407 (2012).

58. Phizicky, E. M. & Fields, S. Protein-protein interactions: Methods for detection and analysis. *Microbiol. Rev.* **59**, 94–123 (1995).

59. Trépout, S. et al. Membrane protein selectively oriented on solid support and reconstituted into a lipid membrane. *Langmuir* **23**, 2647–2654 (2007).

60. Yoneyama, H., Maseda, H., Kamiguchi, H. & Nakae, T. Function of the membrane fusion protein, MexA, of the MexA, B-OprM efflux pump in *Pseudomonas aeruginosa* without an anchoring membrane. *J. Biol. Chem.* **275**, 4628–4634 (2000).

61. Broutin, I. et al. Expression, purification, crystallization and preliminary X-ray studies of the outer membrane efflux proteins OprM and OprN from *Pseudomonas aeruginosa*. *Acta Crystallogr. Sect. F. Struct. Biol. Cryst. Commun.* **F61**, 315–318 (2005).

62. Porte, G. Lamellar phases and disordered phases of fluid bilayer membranes. *J. Phys. Condens. Matter* **4**, 8649–8670 (1992).

63. Strey, R., Jahn, W., Porte, G. & Bassereau, P. Freeze fracture electron microscopy of dilute lamellar and anomalous isotropic (L3) phases. *Langmuir* **6**, 1635–1639 (1990).

64. Pincet, F. et al. FRAP to characterize molecular diffusion and interaction in various membrane environments. *PLoS One* **11**, e0158457 (2016).

## Acknowledgements

We would like to thank Robert S. Hodges for the synthesis of the L₁₂ peptides, José Da Silva Quintas for the technical support. This work utilized facilities supported in part by the Agence Nationale de la Recherche (ANR), the National Science Foundation under Agreement No. DMR-0944772. V.A. is supported by funds from the PhD Program « Frontières du Vivant (FdV) – Cursus Bettencourt ».

## Author contributions

V.A., N.T., F.P. and W.U. made substantial contributions to the conception and design of the work. V.A., N.T., A.V., L.M., M.P., F.P. and W.U. did the experiments. V.A., N.T., F.P. and W.U. participated in the interpretation and visualization of data. V.A. and N.T. have drafted the work. F.P. and W.U. supervised the work. All authors reviewed the manuscript and have approved the submitted version.

## Competing interests

The authors declare no competing interests.

## Additional information

**Supplementary Information** The online version contains supplementary material available at https://doi.org/10.1038/s41598-023-50827-5.

**Correspondence** and requests for materials should be addressed to V.A., F.P. or W.U.

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