Next Article in Journal
Optimization of Castor Oil-Based Ion Selective Electrode (ISE) with Active Agent 1,10-Phenanthroline for Aqueous Pb2+ Analysis
Next Article in Special Issue
Expression of Mutant Glycine Receptors in Xenopus Oocytes Using Canonical and Non-Canonical Amino Acids Reveals Distinct Roles of Conserved Proline Residues
Previous Article in Journal
Profiled Ion-Exchange Membranes for Reverse and Conventional Electrodialysis
Previous Article in Special Issue
Microtransplantation of Postmortem Native Synaptic mGluRs Receptors into Xenopus Oocytes for Their Functional Analysis
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Membranes
Volume 12
Issue 10
10.3390/membranes12100986
membranes-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Review

Xenopus Oocytes as a Powerful Cellular Model to Study Foreign Fully-Processed Membrane Proteins

by
Isabel Ivorra
1,
Armando Alberola-Die
1,
Raúl Cobo
1,
José Manuel González-Ros
2 and
Andrés Morales
1,*
1
Departamento de Fisiología, Genética y Microbiología, Universidad de Alicante, Apdo 99, E-03080 Alicante, Spain
2
Instituto de Investigación, Desarrollo e Innovación en Biotecnología Sanitaria de Elche (IDiBE), Universidad Miguel Hernández, E-03202 Elche, Spain
*
Author to whom correspondence should be addressed.
Membranes 2022, 12(10), 986; https://doi.org/10.3390/membranes12100986
Submission received: 16 September 2022 / Revised: 5 October 2022 / Accepted: 8 October 2022 / Published: 11 October 2022
(This article belongs to the Special Issue The Xenopus Oocyte: A Tool for Membrane Biology)
Browse Figures
Versions Notes

Abstract

:
The use of Xenopus oocytes in electrophysiological and biophysical research constitutes a long and successful story, providing major advances to the knowledge of the function and modulation of membrane proteins, mostly receptors, ion channels, and transporters. Earlier reports showed that these cells are capable of correctly expressing heterologous proteins after injecting the corresponding mRNA or cDNA. More recently, the Xenopus oocyte has become an outstanding host–cell model to carry out detailed studies on the function of fully-processed foreign membrane proteins after their microtransplantation to the oocyte. This review focused on the latter overall process of transplanting foreign membrane proteins to the oocyte after injecting plasma membranes or purified and reconstituted proteins. This experimental approach allows for the study of both the function of mature proteins, with their native stoichiometry and post-translational modifications, and their putative modulation by surrounding lipids, mostly when the protein is purified and reconstituted in lipid matrices of defined composition. Remarkably, this methodology enables functional microtransplantation to the oocyte of membrane receptors, ion channels, and transporters from different sources including human post-mortem tissue banks. Despite the large progress achieved over the last decades on the structure, function, and modulation of neuroreceptors and ion channels in healthy and pathological tissues, many unanswered questions remain and, most likely, Xenopus oocytes will continue to help provide valuable responses.

1. Background

Xenopus laevis, the South African clawed frog, is a laboratory animal that is especially suitable for diverse biological studies since, unlike other anurans, their ovaries always contain oocytes in all stages of development (Figure 1) and new cycles of oogenesis can be initiated during any season by hormonal treatment. In the last five decades, the use of Xenopus oocytes has grown exponentially and has become a chief tool in many laboratories around the world in studies dealing with molecular, cellular, and developmental biology [1,2,3,4,5]. In fact, since the last decade of the 20th century, the Xenopus oocyte constitutes one of the most widely used cell model in molecular biology [3,4]. Furthermore, Xenopus oocytes are particularly useful cells to carry out electrophysiological recordings to study both native ion channels and receptors [6,7] (reviewed in [2,8,9,10]) and foreign proteins transplanted to this convenient host cell after the injection of either the corresponding mRNA or lipid vesicles containing the purified protein (reviewed in [2,9,11,12,13]). Xenopus oocytes have also become the reference model for biophysical studies dealing with structure to function relationships, addressed to unravel the functional consequences of specific mutations of membrane receptors, channels, and transporters (reviewed by [13,14]). Moreover, transplanting foreign, fully-processed membrane proteins to Xenopus oocytes is a methodology more recently used to look deeper into the role played by ion channels and neuroreceptors in the pathogenesis of different diseases as well as for drug screening using electrophysiological recordings and/or fluorescence assays [13,15,16]. Altogether, this has led to the Xenopus oocyte being regarded as a “living test tube” [17].

2. Advantages and Drawbacks of Using Xenopus Oocytes to the Study of Membrane Proteins

As stated by August Krogh [18], an outstanding physiologist awarded the Nobel Prize, for every biological problem there is an organism (model) on which it can be most conveniently studied. In this sense, the Xenopus oocyte model, introduced by Ricardo Miledi, constitutes an excellent paradigm of the Krogh principle to carry out detailed studies on the function of foreign membrane proteins, as was the squid giant axon to understand the ionic basis of the action potential, the frog end-plate junction and the squid stellate ganglion to unveil the basis of synaptic transmission or the Aplysia ganglia, which allowed for the molecular mechanisms of learning and memory to be dealt with. Some of the advantages that the oocyte fulfills to study foreign proteins are:
(a)
Xenopus oocytes have a continuous and asynchronous development, allowing a year-round use of these cells [1].
(b)
Large size, up to 1.3 mm, and roughly spherical shape [1], which facilitates electrophysiological recordings, even allowing the introduction of additional micropipettes for microinjecting compounds [2]. Furthermore, its size enables simultaneous biochemical and optical techniques with quite high spatio-temporal discrimination [19].
(c)
Oocytes constitute an excellent factory for the adequate synthesis and processing of most heterologous proteins [20,21,22,23] (reviewed in [2,13,14,24,25,26,27]).
(d)
These cells are easy to manage and cheap to maintain. Moreover, these cells can be kept alive in an inorganic buffer for long periods (up to several weeks) after their isolation from the ovary, without the need of a specific sterile serum or medium [2,14,16]. Nevertheless, oocytes progressively uncouple from the surrounding follicular cells after their separation from the ovary, losing responsiveness to certain hormones and neurotransmitters.
(e)
The osmotic water permeability of oocytes is quite low (circa 4 × 10−4 cm/s), which allowed for the first functional characterization of exogenous aquaporins [28,29].
(f)
The oocyte plasma membrane can be quite easily isolated either manually ([30,31]; see Figure 1) or by simple biochemical procedures [32]. The isolation of plasma membranes enables one to determine the presence of the microtransplanted protein at the oocyte plasma membrane [31,33] and allows studies concerning both the targeting of membrane proteins and the quantitation of the ratios between functional and the total number of ion channels/receptors incorporated into the cell membrane [12,33,34].
(g)
Although the membrane of Xenopus oocytes might present certain ion channels and receptors, the expression of endogenous proteins from their own mRNA is low (about 5% of their stored mRNA, [13]). Thus the oocyte plasma membrane usually lacks significant levels of neuronal voltage-dependent Na+ and K+ channels and many neuroreceptors and transporters [10].
(h)
The oocyte has powerful intracellular signaling cascades, mostly involving InsP3 synthesis and Ca2+ release from intracellular stores after phospholipase-C activation. Thus, heterologous expression of certain metabotropic receptors can be simply monitored by recording Ca2+-dependent Cl− currents, since the Ca2+-dependent Cl− channel, anoctamin 1 (TMEM16A), is highly expressed in the oocyte membrane [2,27,35,36].
(i)
Oocytes are convenient cells to screen potential drugs and to determine their relative efficacies against specific targets. These studies have been boosted by the introduction of devices for the automated voltage-clamping of these cells [13,16].
Nevertheless, Xenopus oocytes also present some disadvantages when studying membrane proteins including:
(a)
In the ovary, oocytes are found as follicles, constituted by several cellular and acellular layers surrounding the oocyte, from inner to outer: (i) the oocyte; (ii) a fibrous vitelline membrane; (iii) a monolayer of follicular cells, which is coupled to microvilli of the oocyte membrane by gap junctions [37]; (iv) a theca, containing mainly collagen, fibrocytes and small blood vessels; and (v) a layer of epithelial cells. The layers surrounding the oocyte might constitute a handicap to study certain transplanted proteins since follicular cells express ion channels and receptors of their own and are electrically coupled to the oocyte. However, the layers surrounding the oocyte can be removed either manually or by enzymatic means.
(b)
There is a certain variability in the expression efficiency of oocytes, which has been related to seasonal differences [27]. Actually, some laboratories stop working with oocytes during summer because of their low quality. Furthermore, noise and other vibrations should be restricted around aquarium facilities since Xenopus are quite sensitive to them.
(c)
As previously mentioned, oocytes randomly express certain ion channels and receptors, which might be confused with those heterologously expressed [13]. Thus, it becomes necessary to keep in mind the channels and receptors that can be endogenously expressed by oocytes (excellent reviews regarding this issue are provided in [2,8,9,10,24,25]), though some of them can be pharmacologically blocked. Nevertheless, other cell models commonly used for the heterologous expression of ion channels and transporters such as human embryonic kidney cells (HEK) also have endogenous ion channels [38].
(d)
The large size of the oocyte together with the presence of several surrounding layers (cellular and acellular) constitute a limitation to obtaining fast ligand-applications, particularly when using large molecules [39], and consequently, to record fast-kinetics currents (it hinders the resolution of ligand-elicited currents at resolutions below hundred milliseconds; [40]). Moreover, when follicular cells remain attached to the oocyte, certain measured pharmacological values (i.e., half maximal effective concentration, EC50, or half maximal inhibitory concentration, IC50) might be inaccurate [39]. In addition, several factors such as the oocyte large size, the presence of numerous microvilli at its plasma membrane, and its electrical coupling to follicular cells contribute to eliciting extremely large capacitive artifacts, which prevent resolving fast voltage-dependent currents below a few milliseconds [14].

3. Transplant of Fully Processed Membrane Proteins to the Xenopus Oocyte

As previously indicated, Xenopus oocytes have allowed for the biophysical characterization of many ion channels, neurotransmitter receptors, and transporters thanks to their ease of use, amenability for electrophysiological recordings and their capability to efficiently and faithfully translate most heterologous mRNAs (reviewed in [2,24,25]). It is known that Xenopus oocytes are able to make many post-translational modifications of the proteins coded by the exogenous mRNA (as glycosylation, phosphorylation, acetylation, or folding), and to correctly assemble oligomeric receptor/channel complexes. However, occasionally, they do not mimic the post-translational modifications carried out by the cells that used to express them natively. Most likely, these differences account for the failed or altered function of some foreign proteins expressed in oocytes and, perhaps, also for the variability observed between oocytes [27]. For instance, Torpedo nicotinic acetylcholine (ACh) receptors (nAChRs) expressed in oocytes after injecting the corresponding mRNAs have an altered pattern of glycosylation [41], and neuronal sympathetic nAChRs (α3β4 and α4β4 subunits) do not exhibit certain properties of the native receptors, putatively because oocytes fail to correctly assemble their different subunits or because of the post-translational channel modifications [42]. Similarly, native brain and heterologously expressed rat α4β2 nAChRs showed significant pharmacological differences [43]. In this regard, it should be considered that certain membrane proteins including ion channels are modulated by their interaction with accessory subunits, which might be lacking in the host cell membrane and are not incorporated when mRNA is used to express specific foreign proteins in the oocyte [13,27,43,44]. Additionally, specific lipid requirements of certain membrane proteins might constitute a severe handicap to the faithful functional expression of some heterologous proteins [45]. Moreover, it has been shown that different mutations in the M4 (the outermost lipid-facing α-helix of the transmembrane domain) of α4β2 nAChRs reduced or abolished the function of these receptors when expressed in the HEK cells, but not when expressed in Xenopus oocytes [46]. The differences in the functional activity of these mutant nAChRs between both cell types seem to be due to the different lipid composition of their respective plasma membranes [46].
The above-mentioned handicaps were overcome when Marsal et al. [47] found that foreign membranes carrying neurotransmitter receptors and ion channels could be incorporated into the Xenopus oocyte membrane, which allowed for the microtransplantation of fully processed proteins retaining their natural environment. Since then, several groups have followed this approach of the intracellular injection of plasma membranes to study foreign membrane proteins in Xenopus oocytes (reviewed in [12]). Thus, many neuroreceptors, transporters, and ion channels have been transplanted from their original cells to the oocyte membrane including: (i) nAChRs from Torpedo electroplaques [33,47], muscle fibers [48,49], brain neurons [50], and from cell lines overexpressing heterologous neuronal nAChRs [26]; (ii) gamma-aminobutyric acid receptor type A (GABAAR) from the brain synaptosomal membranes [15,26,51,52,53,54,55,56,57,58,59,60,61]; (iii) glutamate (AMPA, α-amino-3-hydroxy-5-methyl-4-isoxazolepropionic acid/Kainate/NMDA, N-methyl-D-aspartate) receptors [26,52,62,63,64]; (iv) voltage-activated Na+ and Ca2+ channels from the human brain [34,65]; (v) Cl− channels from Torpedo electroplax [33,47] and from human syncytiotrophoblast microvillous membranes [66]; and (vi) membrane transporters such as P-glycoprotein [31] and the Cl− transporters, KCC1 (K+–Cl− cotransporter type 1) and NKCC2 (Na+–K+–Cl− cotransporter type 2; [55]).
The intracellular injection of plasma membranes to insert foreign proteins into the oocyte membrane was later extended by microtransplanting functional proteins after their purification and reconstitution in lipid vesicles of defined composition [33,67,68,69]. The main steps followed to microtransplant purified and reconstituted nAChRs from Torpedo electroplaques to the Xenopus oocyte membrane are shown in Figure 2.
It should be noted that the goal of this experimental approach is not to use oocytes as a factory to generate proteins, but as a convenient cellular system to carry out detailed functional studies of the transplanted membrane proteins. Nevertheless, the use of purified and reconstituted proteins, instead of fragments of cellular membranes, has several advantages including: (i) it allows for the study of single molecular entities; (ii) it does not require the transplanted protein to be highly expressed in the plasma membrane, although the presence of a large amount of protein simplifies its purification; and (iii) it makes it possible to study the influence that the lipid composition of the reconstitution matrix has on both the function of the transplanted protein and the process of fusion between the vesicular and cellular membranes. This later point is of special relevance since many proteins need to interact with specific lipids for developing their full functional activity [70,71]. Consequently, the microtransplantation of purified and reconstituted proteins into the Xenopus oocyte membrane arises as an excellent way to unravel the lipid–protein interactions, since it allows us to both insert proteins bound to specific lipids, which can even be labelled, and to selectively modify the lipid content of the cell membrane. Using this approach, it is possible to change not only the ratio of different phospholipids surrounding the protein to determine their functional relevance, but also the charge or the length of the acyl chains to induce local changes in the bilayer thickness and elasticity, which might also be important for the protein activity [72,73]. Thus, this approach constitutes a very useful extension to the classical use of cDNA or mRNA for the functional study of ion channels and neurotransmitter receptors.

3.1. Characteristics of Protein Microtransplantation to the Oocyte Plasma Membrane

3.1.1. Proteoliposome-Plasma Membrane Fusion Does Not Require an Intracellular Ca2+ Increase

Several factors have been proposed to facilitate the fusion of artificial and cellular membranes including osmolarity, pH, lipid composition, and particularly, the presence of some “fusion factors” including certain proteins and Ca2+. Lipid bilayers can fuse together passively in the absence of Ca2+, but many membrane-fusion processes such as neurotransmitter and hormonal secretion, myoblast fusion, membrane resealing, and nuclear vesicle fusion in Xenopus eggs either require or are boosted by an increase in the intracellular Ca2+ concentration ([Ca2+]i). The role played by [Ca2+]i in the efficacy of transplanting purified proteins into the Xenopus oocyte membrane has been explored [74]. In these experiments, [Ca2+]i was decreased by using Ca2+ chelators, either through preincubating oocytes with 1,2-bis (2-aminophenoxy)ethane N,N,N′,N′-tetraacetic acid acetoxymethyl ester (BAPTA-AM) or loading the cells with ethyleneglycol-bis (β-aminoethylether)-N,N,N′,N′-tetraacetic acid (EGTA), and several hours later, these cells were injected with proteoliposomes bearing nAChRs. Effective Ca2+ chelation was proven by the lack of oscillatory Ca2+-dependent Cl− currents after superfusing these cells with serum, which activates lysophosphatidic acid receptors of the oocyte membrane [75,76] and, subsequently, the phosphatidylinositol cascade (Figure 3; [74]). These experiments evidenced that both the control and Ca2+-chelated oocytes presented similar ACh-elicited currents (IAChs), indicating that the fusion of the proteoliposome vesicle with the cellular membrane was not dependent on the local increases of [Ca2+]i. Nevertheless, the IAChs elicited in oocytes loaded with either BAPTA-AM or EGTA were slightly smaller than those in the control cells. A lower incorporation of neuroreceptors after synaptosomal membrane injection has also been reported when the oocytes were loaded with Ca2+-chelators [61]. It has been suggested that the smaller responses might be related to a slower trafficking of lipid vesicles or, alternatively, to alteration in the binding of the injected vesicles to the plasma membrane [74]. Although a [Ca2+]i increase must occur when rupturing the oocyte membrane by the needle when injecting the proteoliposomes, it seems that this transient [Ca2+]i increase does not account for the fusion of proteoliposomes to the oocyte membrane. In concordance with this, the incorporation of new nAChRs to the oocyte membrane takes place for many hours after proteoliposome injection, when [Ca2+]i should be returned to very low levels in the Ca2+-chelated groups.

3.1.2. Microtransplanted Proteins Are Incorporated in Patches

Proteoliposomes bearing reconstituted membrane proteins are microinjected focally into the oocyte, usually at the vegetal hemisphere, to avoid damaging the large nucleus of these cells, located close to the animal pole. Thus, the question is whether the inserted proteins incorporate to the oocyte membrane close to the injection site or, instead, they spread along the oocyte surface. To answer this question, two different experimental approaches have been used: (i) focal recordings mapping the oocyte surface, looking for activity of the transplanted receptors [67]; and (ii) imaging the microtransplanted receptors on the oocyte surface by using fluorescent probes [12,34,47,62,69]. Both techniques showed that either the plasma membranes or purified and reconstituted receptors incorporated in patches into the oocyte membrane, with the density and size of the patches being larger close to the injection site, but they were widely distributed along the oocyte surface. It has been estimated that the total extent of the patches of fluorescent-stained plasma membrane might reach up to 20% of the oocyte surface [62]. In concordance with these observations, functional patches of nAChRs could be found in the animal hemisphere after injecting proteoliposomes at the vegetal hemisphere [67]. This patchy incorporation of the microtransplanted nAChRs could also be evidenced by superfusing the whole oocyte with ACh while recording the IAChs. As shown in Figure 4, the elicited IAChs commonly showed one or several “humps” during their activation phase, most likely due to the successive activation of patches located around the oocyte surface.

3.1.3. Proteoliposomes of Different Lipid Composition Allow Functional nAChR Microtransplantation

The microtransplant of purified and reconstituted membrane proteins to oocytes allows these proteins to be embedded in specific lipid matrices. The relevant role played by the lipid composition in the mechanisms of membrane fusion is well-established. Furthermore, lipids are crucial in both determining the membrane structure and dynamics and in modulating membrane proteins by specific interactions [46,77,78,79]. Thus, purified nAChRs were reconstituted in different lipid matrices including mixtures of asolectin (Aso), neutral phospholipids such as phosphatidylcholine (PC), anionic phospholipids such as phosphatidic acid (PA), and cholesterol (Chol), and the resulting proteoliposomes were injected into the oocytes. These experiments showed that nAChRs embedded in diverse lipid matrices were functionally transplanted to the oocyte membrane ([68]; see below). This is a quite interesting finding, since nAChRs reconstituted in vesicles of pure PC lost their ability to support cation channel activity [80,81] (reviewed in [82,83]). Therefore, it seems that nAChRs microtransplanted to the oocyte become surrounded, at least in part, by lipids from their own cell membrane. Consequently, when considering the efficiency of functional nAChR transplantation, the role played by the reconstitution lipid composition in the proteoliposome-oocyte membrane fusion is somehow overshadowed by the subsequent lipid exchange taking place around the microtransplanted protein, which is capable, in some way, of customizing its environment, likely by the lateral segregation of specific lipids [78,82,84,85].

3.2. Advantages and Limitations of Transplanting Purified Proteins Reconstituted in Artificial Lipid Bilayers

An additional advantage of using Xenopus oocytes as the host cell for the functional and biophysical studies of heterologous proteins is that their membrane lipid composition is well-known [86,87], and furthermore, it can be customized to some extent. Thus, the Chol to phospholipid (PL) molar ratio (Chol/PL) in the oocyte membrane (roughly 0.5) can almost be duplicated by incubating oocytes in a solution containing Chol-enriched liposomes. Interestingly, Chol plays a key role in the function of nAChRs, and even Chol rich microdomains may promote cooperativity between neighboring receptors [78,79,88,89]. In fact, Torpedo postsynaptic membranes are particularly rich in Chol [78,79,90] and Chol is required for normal functionality of this receptor [91,92,93]. Conversely, the Chol/PL ratio can be decreased, for instance, by incubating oocytes with methyl-β-cyclodextrin [94]. Likewise, the membrane lipid content in the oocyte membrane can be altered by either incubating oocytes with lipid-defined liposomes or activating specific pathways of lipid metabolism. When changing the membrane lipid composition, it should be considered that certain lipids are charged molecules and hence their presence in the oocyte membrane might modulate the function of some microtransplanted proteins, particularly ion channels, by specific interactions (see below), but also by electrostatic mechanisms. Therefore, it is well-known that the biophysical properties of ion channels can be modulated by electrostatic charges present either in the protein itself or in nearby molecules (i.e., the surrounding phospholipids) [70,95,96].
There are also certain handicaps related to this technique of microtransplanting purified and reconstituted proteins to the Xenopus oocyte membrane including:
(a)
Incorrect orientation of the incorporated proteins in the oocyte plasma membrane. Although the microtransplantation of foreign membrane proteins allows several million nAChRs to be functionally incorporated, the overall efficiency of this approach is, at least for certain proteins, rather low, considering the amount of injected protein [33,67]. Noticeably, membrane proteins of different sizes and shapes might generate proteoliposomes with different protein orientations during the process of detergent dialysis [97]. Therefore, it could be that some of the microtransplanted nAChRs were incorporated into the oocyte membrane in the “wrong” orientation, hence being functionally silent (see Figure 5). It is possible to determine the orientation of the microtransplanted nAChRs in oocytes by combining electrophysiological and binding techniques. These experiments showed the following. (i) Roughly 90% of the microtransplanted nAChRs were incorporated into the oocyte membrane with the binding domain facing up to the cytoplasm [33]. This outside-in orientation of nAChRs in the oocyte membrane could account for the low efficiency of functional nAChR microtransplantation, since nAChRs incorporated with the “wrong” orientation lost their functional activity (Figure 5; [67]). Interestingly, most nAChRs in proteoliposomes are oriented outside-out [91], but fusion of proteoliposomes with the cell membrane commonly results in an inverted protein orientation (see Figure 5; [98]). (ii) The proportion of the incorporated versus injected nAChRs, determined at a fixed time, reached up to 3%, indicating that the fusion of proteoliposomes with the cell membrane is quite an efficient process [33]. Moreover, other membrane proteins such as Torpedo Cl− channels (ClC0) were functionally incorporated in the oocyte plasma membrane much more efficiently than nAChRs [33]. Remarkably, a protein change in orientation within the lipid bilayer (protein-flipping) can be triggered, at least in certain proteins, by modifying the lipid composition of the bilayer, both in vitro and in vivo [99].
(b)
Presence of multilamellar proteoliposomes. Proteoliposomes bearing purified membrane proteins are commonly obtained by detergent removal dialysis [67,69]. Many of the proteoliposomes harvested under these experimental conditions are multilamellar, particularly when large proteins such as the nAChR are incorporated into liposomes. This constitutes a handicap since the presence of multilamellar proteoliposomes might affect both the protein function and its incorporation to the oocyte plasma membrane. To diminish this handicap, the harvested multilamellar proteoliposomes should be broken into smaller unilamellar vesicles, prior to injecting the sample into the oocytes. This can be attained by sonication of the sample in a water bath until the suspension becomes homogenized and less turbid [67,100,101]. Alternatively, small unilamellar proteoliposomes of homogenous sizes can be obtained from multilamellar vesicles by using a mini-extruder [102].
(c)
Microtransplanted proteins do not always remain surrounded by the original proteoliposome lipids. As above-mentioned, some lipid exchange might take place around the protein, as evidenced by the functional recovery of nAChR reconstituted in PC when microtransplanted to the oocyte membrane.

4. Microtransplanting nAChRs to the Xenopus Oocyte Membrane as a Useful Approach to Study Lipid–Protein Interactions

The relevance of the interaction between proteins and their surrounding membrane lipids has been reinforced in the last few decades. As above-mentioned (see Section 3.1.3), several in vitro studies have shown that nAChRs are fully functional when reconstituted in a heterogeneous mixture of phospholipids such as that provided by crude soybean (Aso) lipids. Furthermore, these studies indicate that PA and Chol play a major role in preserving the functional activity of this protein. Conversely, when nAChRs are reconstituted in plain PC bilayers, their functional activity is completely lost [80,81,91] (reviewed in [83]), even with Chol restoration [81,92,93]. Taking advantage of the fact that nAChRs can be microtransplanted to the Xenopus oocyte membrane after intracellular injection of proteoliposomes, it is possible to determine the effect of the reconstitution lipid matrix on the functional properties of the transplanted nAChRs. Thus, nAChRs were reconstituted in either asolectin (R-Aso), PC:Chol (75:25 molar ratio; R-PC+Chol) or a mixture of PA:PC:Chol (25:50:25 molar ratio; R-PA+PC+Chol). Oocyte injection of nAChR proteoliposomes reconstituted in any of these lipid matrices rendered functional nAChRs in the oocyte membrane (Figure 6A). Interestingly, IAChs were significantly larger in oocytes injected with R-PA+PC+Chol than when injected either with R-Aso or R-PC+Chol (Figure 6A; [68]). These larger IAChs in R-PA+PC+Chol injected oocytes might be due to either an enhanced fusion of these proteoliposomes with the oocyte plasma membrane or to an increased activity of the nAChRs when surrounded by PA+PC+Chol lipids. To assess whether this IACh increase is due to a direct effect of the lipid matrix, some oocytes were pre-injected with plain liposomes of either Aso (control liposomes), egg-PA (PA), or a mixture of PA:PC:Chol (25:50:25) 6 h before injecting into the oocyte R-Aso proteoliposomes (see Figure 6B). Noticeably, the oocytes pre-injected with either PA or PA:PC:Chol elicited larger IAChs than those of control oocytes (injected with Aso-liposomes), indicating that PA modulates nAChR function [68,92]. In agreement with this, it is remarkable that the nAChR induces, by itself, the formation of specific PA-rich lipid domains in the membrane vesicles [85]. Moreover, this hypothesis is further supported by the fact that the more nAChR is purified from Torpedo electroplaques, the greater the PA proportion is obtained in the membrane fraction, increasing from 0.5 to 1.6% up to 2.2–2.9% of the total lipids [90]. Interestingly, PA is known to enhance the function of other ion channels, as the KcsA, a potassium channel from the Streptomyces lividans [83,103,104]. In addition, an enhanced fusion of R-PA+PC+Chol proteoliposomes with the cell membrane was discarded because the incorporation of ClC-0 channels (a minor contaminant in some of the injected samples; [33]) was similar when the oocytes were injected with either the R-Aso, R-PC+Chol, or R-PA+PC+Chol proteoliposomes [68].
As above indicated, nAChRs reconstituted in the liposomes of just PC:Chol lacked functional activity [81], but these receptors recovered their full-activity as ion channels after injecting these proteoliposomes into the oocyte (Figure 6A). This functional recovery suggests that the system is sufficiently dynamic to allow for the exchange of lipids between the proteoliposome and their own oocyte membrane. Noticeably, the oocyte plasma membrane has a higher proportion of Chol than phospholipids [45,46], and Chol plays an essential role in preserving nAChR function [89]. Then, why did the oocytes injected with nAChR reconstituted in PA display larger currents? This is most likely because of the tight binding of PA to nAChR, hindering its free exchange with other bulk membrane lipids [90], even leading to the formation of a PA microdomain around the nAChR [85]. This suggested explanation implies that PA acts as a positive modulator of nAChR, enhancing its functional activity [68].

5. Use of Microtransplanted Proteins to Study Functional and Pharmacological Properties of Ion Channels and Receptors

Transplanting fully-processed foreign membrane proteins to the Xenopus oocyte membrane constitutes a valuable approach to carry out detailed functional and biophysical studies on neuroreceptors and other ion channels, preserving their native conformation. After confirming that purified and reconstituted nAChRs microtransplanted to the oocyte membrane preserve their native biophysical properties [67], this technique has been used to study the modulation of this complex protein by different molecules of therapeutic relevance. Thus, this experimental approach has been used to assess the allosteric modulation of muscle-type nAChR function by several cholinesterase inhibitors [105,106], local anesthetics such as lidocaine [107] or akin molecules [59,60], tetracaine [108], and benzocaine [109] or natural anti-inflammatory agents such as peimine [110]. By combining electrophysiological and virtual docking assays, it has been possible to identify specific nAChR residues interacting with different drugs, which support the open-channel blockade elicited by either lidocaine or diethylamine, a molecule resembling the hydrophilic moiety of lidocaine [59,107,110] or tetracaine [108]. Although the kinetic changes elicited by superfusing Xenopus oocytes with modulating drugs are rather slow (usually over 1 s; see above the section of drawbacks of using Xenopus oocytes to study membrane proteins), the kinetics of the open-channel blockade can be resolved at much higher resolution. Since quaternary-ammonium cholinesterase inhibitors and many local anesthetics are positively charged molecules, the application of positive voltage pulses removes the drug from the channel, thus unplugging the pore by electrostatic repulsion. If the oocyte is maintained in the presence of ACh and the open-channel blocker, the sudden return of the cell membrane potential to negative values, after the application of a strong positive pulse to vanish the open-channel blockade, allows one to determine the kinetics of open-channel blockade with a fairly high temporal resolution [108,110]. Furthermore, the fraction of the voltage field (δ), sensed by the drug at its binding site, can be computed by using the Woodhull equation [111] to electrophysiologically estimate the loci where these open-channel blockers bind within the channel pore [106,107]. Several of the therapeutic molecules tested boosted nAChR desensitization, for instance, tetracaine, most likely acting on residues that are shallowly located in the channel pore [108]. Noteworthy, changes in nAChR desensitization are easier to compute by using oocyte voltage-clamping than by single-channel recording. Since desensitization increases the affinity of nAChR to ACh, the extent of desensitization can be easily determined by comparing the deactivation kinetics of IAChs when the modulatory drug is either present or absent [108,110]. In addition, some of these drugs act on nAChRs outside the channel pore, mostly at either the extracellular domain or the transmembrane domain at the inter- or intra-subunit crevices. Drug binding to this loci located outside the channel pore can account for the closed-channel blockade, usually elicited at concentrations higher than those required for open-channel blockade [107,108,110].
Remarkably, plasma membranes from either healthy or diseased human postmortem brains (from tissue banks) and other tissues have been successfully microtransplanted to the Xenopus oocyte membrane, where the functional and biophysical properties of their neurotransmitter receptors and other ion channels can be studied in detail [12,52,58,66]. Furthermore, this new approach makes the microtransplantation of fully-processed membrane proteins a valuable method to gain insights into the knowledge of the molecular alterations present in specific neurological disorders including Alzheimer, epilepsy, autism, or amyotrophic lateral sclerosis [13,49,53,54,55,56,57,58,65], but also as a powerful and specific way to explore the effects of putative therapeutic molecules and newly designed drugs on native human targets [12,58]. In addition, the microtransplantation procedure has also been probed as a toxicologically-relevant ex vivo assay. Therefore, the effects of neurotoxic insecticides such as DDT (dichlorodiphenyltrichloroethane) on the voltage-dependent Na+ channels from rat brain membranes have been successfully tested [34]. A striking advantage of this methodology is that not only can the properties and behavior of the matured membrane proteins be easily studied with diverse techniques, they can also be functionally characterized together with the lipids and other proteins that constituted its natural environment, which might alter or modulate the transplanted protein properties [44].
Although the study of foreign membrane proteins microtransplanted to the Xenopus oocyte suffer from certain handicaps, as stated above, this procedure constitutes, as of today, one of the finest approaches to carry out detailed functional studies on native, fully-processed, heterologous membrane proteins from different sources including human tissues and, furthermore, it constitutes an exceptional test bank to assay new medicinal drugs.

6. Conclusions and Future Perspectives

Xenopus oocytes have become a valuable tool to study the function and modulation of foreign proteins for over four decades and, most likely, they will continue to be worthy for this purpose for many more years. Thus, there are still many relevant biological problems unsolved that can be best addressed by microtransplanting foreign membrane proteins to this host cell, where they can be more easily studied. For instance, (i) to unravel the modulating effects of specific membrane-lipids on the function of different membrane proteins including pumps, receptors, and ion channels. Actually, thus far, most of the studies dealing with the functional and structural modulation of neuroreceptors and ion channels by their surrounding lipids have been carried out on artificial membranes. Thus, the introduction of novel methods is required to study the lipid–protein interactions in native cell membranes, which might confirm, or not, the previous results found in artificial systems. (ii) To explore the targeting of foreign proteins to the cell membrane, which might be particularly relevant for mutated proteins and the scaffolding by other molecules surrounding the mature membrane protein. (iii) To assess the mechanisms of the dysfunction of membrane proteins obtained from pathological tissue banks. Actually, transplanting receptors and ion channels from human post-mortem tissues from individuals either healthy or suffering specific diseases might be considered as a “Rosetta stone” for the analysis of human membrane protein function [112], and the transplanted proteins should constitute an exceptional target for assaying new molecules designed to modulate specific proteins. (iv) To gain a deeper insight into the mechanisms by which new targeted molecules modulate the function of transplanted membrane proteins. (v) As a cell model to study the mechanisms underlying the constitutive fusion of membranes. (vi) As a suitable cell to study mutated receptors or ion channels overexpressed in convenient cell lines.
Although our knowledge on the structure, function, and modulation of neuroreceptors and ion channels in healthy and pathological tissues has been greatly expanded over the last decades, many unanswered questions remain and, most likely, the Xenopus oocytes will continue helping to provide valuable responses.

Author Contributions

Writing—original draft preparation, I.I. and A.M.; writing—review and editing, I.I., A.A.-D., R.C., J.M.G.-R. and A.M. All authors have read and agreed to the published version of the manuscript.

Funding

The work in the authors’ laboratories has been supported by grants SAF2017-82977-P (AEI/FEDER, UE) and PGC2018-093505-B-I00 from MINECO and GRE17-01 from Universidad de Alicante (Spain).

Institutional Review Board Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

Abbreviations

AchAcetylcholine;
AMPAα-amino-3-hydroxy-5-methyl-4-isoxazolepropionic acid;
BAPTA-AM1,2-bis (2-aminophenoxy)ethane N,N,N′,N′-tetraacetic acid acetoxymethyl ester
ClC0Chloride channel type 0 (Torpedo)
CholCholesterol
Chol/PLCholesterol to phospholipid molar ratio
δFraction of the voltage field sensed by a drug in the membrane
DDTDichlorodiphenyltrichloroethane
EGTAEthyleneglycol-bis (β-aminoethylether)-N,N,N′,N′-tetraacetic acid
EcExtracellular side
EC50Half maximal effective concentration
GABAARGamma-aminobutyric acid receptor type A
HEK (HEK 293)Human embryonic kidney 293 cells
IAChACh-elicited current
IC50Half maximal inhibitory concentration
InsP3Inositol 1,4,5-trisphosphate
IcIntracellular side
[Ca2+]i Intracellular Ca2+ concentration
KCC1 K+–Cl− cotransporter type 1
nAChRNicotinic acetylcholine receptor
NMDAN-methyl-D-aspartate
PAPhosphatidic acid
PCPhosphatidylcholine
KcsAA potassium channel from the Streptomyces lividans
R-AsoProteoliposome of asolectin bearing nAChRs
R-PA+PC+CholProteoliposome of PA, PC and Chol bearing nAChRs
R-PC+CholProteoliposome of PC and Chol bearing nAChRs
NKCC2Na+–K+–Cl− cotransporter type 2
TMEM16ACa2+ activated Cl− channel, anoctamin1

References

  1. Dumont, J.N. Oogenesis in Xenopus laevis (Daudin). I. Stages of oocyte development in laboratory maintained animals. J. Morphol. 1972, 136, 153–179. [Google Scholar] [CrossRef] [PubMed]
  2. Miledi, R.; Parker, I.; Sumikawa, K. Transplanting receptors from brains into oocytes. In FIDIA Research Foundation Neuroscience Award Lectures; Raven Press, Ltd.: New York, NY, USA, 1989; Volume 3, pp. 57–90. [Google Scholar]
  3. Gurdon, J.B. Introductory comments: Xenopus as a laboratory animal. In The Biology of Xenopus; Tinsley, R.C., Kobel, H.R., Eds.; Clarendon Press: Oxford, UK, 1996; pp. 3–6. [Google Scholar]
  4. Mowry, K.L. Using the Xenopus Oocyte Toolbox. Cold Spring Harb. Protoc. 2020, 4, 095844. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. De Robertis, E.M.; Gurdon, J.B. A Brief History of Xenopus in Biology. Cold Spring Harb. Protoc. 2021, 12, 107615. [Google Scholar] [CrossRef] [PubMed]
  6. Kusano, K.; Miledi, R.; Stinnakre, J. Acetylcholine receptors in the oocyte membrane. Nature 1977, 270, 739–741. [Google Scholar] [CrossRef]
  7. Kusano, K.; Miledi, R.; Stinnakre, J. Cholinergic and catecholaminergic receptors in the Xenopus oocyte membrane. J. Physiol. 1982, 328, 143–170. [Google Scholar] [CrossRef]
  8. Dascal, N. The use of Xenopus oocytes for the study of ion channels. Crit. Rev. Biochem. Mol. Biol. 1987, 22, 317–387. [Google Scholar] [CrossRef]
  9. Sobczak, K.; Bangel-Ruland, N.; Leier, G.; Weber, W.M. Endogenous transport systems in the Xenopus laevis oocyte plasma membrane. Methods 2010, 51, 183–189. [Google Scholar] [CrossRef]
  10. Martinez-Torres, A.; Pereida-Jaramillo, E. The use of Xenopus oocytes to study the biophysics and pharmacological properties of receptors and channels. In Xenopus: From Basic Biology to Disease Models in the Genomic Era; Fainsod, A., Moody, S.A., Eds.; CRC Press: Boca Raton, FL, USA, 2022; pp. 143–151. [Google Scholar] [CrossRef]
  11. Weber, W.M. Ion currents of Xenopus laevis oocytes: State of the art. Biochim. Biophys. Acta 1999, 1421, 213–233. [Google Scholar] [CrossRef] [Green Version]
  12. Eusebi, F.; Palma, E.; Amici, M.; Miledi, R. Microtransplantation of ligand-gated receptor-channels from fresh or frozen nervous tissue into Xenopus oocytes: A potent tool for expanding functional information. Prog. Neurobiol. 2009, 88, 32–40. [Google Scholar] [CrossRef]
  13. Zeng, S.L.; Sudlow, L.C.; Berezin, M.Y. Using Xenopus oocytes in neurological disease drug discovery. Expert Opin. Drug Discov. 2020, 15, 39–52. [Google Scholar] [CrossRef]
  14. Stühmer, W.; Parekh, A.B. Electrophysiological recordings from Xenopus oocytes. In Single-Channel Recording; Sakmann, B., Neher, E., Eds.; Springer: Boston, MA, USA, 1995; pp. 341–356. [Google Scholar] [CrossRef]
  15. Palma, E.; Trettel, F.; Fucile, S.; Renzi, M.; Miledi, R.; Eusebi, F. Microtransplantation of membranes from cultured cells to Xenopus oocytes: A method to study neurotransmitter receptors embedded in native lipids. Proc. Natl. Acad. Sci. USA 2003, 100, 2896–2900. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Kvist, T.; Hansen, K.B.; Bräuner-Osborne, H. The use of Xenopus oocytes in drug screening. Expert Opin. Drug Discov. 2011, 6, 141–153. [Google Scholar] [CrossRef] [PubMed]
  17. Gurdon, J.B.; Wickens, M.P. The use of Xenopus oocytes for the expression of cloned genes. Methods Enzym. 1983, 101, 370–386. [Google Scholar] [CrossRef]
  18. Krogh, A. The progress of Physiology. Science 1929, 70, 200–204. [Google Scholar] [CrossRef]
  19. Demuro, A.; Parker, I. Optical single-channel recording: Imaging Ca2+ flux through individual N-type voltage-gated channels expressed in Xenopus oocytes. Cell Calcium 2003, 34, 499–509. [Google Scholar] [CrossRef]
  20. Gurdon, J.B.; Lane, C.D.; Woodland, H.R.; Marbaix, G. Use of frog eggs and oocytes for the study of messenger RNA and its translation in living cells. Nature 1971, 233, 177–182. [Google Scholar] [CrossRef]
  21. Barnard, E.A.; Miledi, R.; Sumikawa, K. Translation of exogenous messenger RNA coding for nicotinic acetylcholine receptors produces functional receptors in Xenopus oocytes. Proc. R. Soc. Lond. Ser. B. Biol. Sci. 1982, 215, 241–246. [Google Scholar] [CrossRef]
  22. Miledi, R.; Parker, I.; Sumikawa, K. Properties of acetylcholine receptors translated by cat muscle mRNA in Xenopus oocytes. EMBO J. 1982, 1, 1307–1312. [Google Scholar] [CrossRef]
  23. Noda, M.; Ikeda, T.; Suzuki, H.; Takeshima, H.; Takahashi, T.; Kuno, M.; Numa, S. Expression of functional sodium channels from cloned cDNA. Nature 1986, 322, 826–828. [Google Scholar] [CrossRef]
  24. Soreq, H.; Seidman, S. Xenopus oocyte microinjection: From gene to protein. Methods Enzym. 1992, 207, 225–265. [Google Scholar] [CrossRef]
  25. Miller, A.J.; Zhou, J.J. Xenopus oocytes as an expression system for plant transporters. Biochim. Biophys. Acta 2000, 1465, 343–358. [Google Scholar] [CrossRef] [Green Version]
  26. Miledi, R.; Palma, E.; Eusebi, F. Microtransplantation of neurotransmitter receptors from cells to Xenopus oocyte membranes: New procedure for ion channel studies. Methods Mol. Biol. 2006, 322, 347–355. [Google Scholar] [CrossRef]
  27. Terhag, J.; Cavara, N.A.; Hollmann, M. Cave Canalem: How endogenous ion channels may interfere with heterologous expression in Xenopus oocytes. Methods 2010, 51, 66–74. [Google Scholar] [CrossRef] [PubMed]
  28. Zhang, R.B.; Logee, K.A.; Verkman, A.S. Expression of mRNA coding for kidney and red cell water channels in Xenopus oocytes. J. Biol. Chem. 1990, 265, 15375–15378. [Google Scholar] [CrossRef]
  29. Preston, G.M.; Carroll, T.P.; Guggino, W.B.; Agre, P. Appearance of water channels in Xenopus oocytes expressing red cell CHIP28 protein. Science 1992, 256, 385–387. [Google Scholar] [CrossRef] [Green Version]
  30. Sadler, S.E.; Maller, J.L. Progesterone inhibits adenylate cyclase in Xenopus oocytes. Action on the guanine nucleotide regulatory protein. J. Biol. Chem. 1981, 256, 6368–6373. [Google Scholar] [CrossRef]
  31. Aleu, J.; Ivorra, I.; Lejarreta, M.; González-Ros, J.M.; Morales, A.; Ferragut, J.A. Functional incorporation of P-glycoprotein into Xenopus oocyte plasma membrane fails to elicit a swelling-evoked conductance. Biochem. Biophys. Res. Commun. 1997, 237, 407–412. [Google Scholar] [CrossRef] [Green Version]
  32. Leduc-Nadeau, A.; Lahjouji, K.; Bissonnette, P.; Lapointe, J.Y.; Bichet, D.G. Elaboration of a novel technique for purification of plasma membranes from Xenopus laevis oocytes. Am. J. Physiol. Cell Physiol. 2007, 292, C1132–C1136. [Google Scholar] [CrossRef]
  33. Ivorra, I.; Fernández, A.; Gal, B.; Aleu, J.; González-Ros, J.M.; Ferragut, J.A.; Morales, A. Protein orientation affects the efficiency of functional protein transplantation into the Xenopus oocyte membrane. J. Membr. Biol. 2002, 185, 117–127. [Google Scholar] [CrossRef]
  34. Murenzi, E.; Toltin, A.C.; Symington, S.B.; Morgan, M.M.; Clark, J.M. Evaluation of microtransplantation of rat brain neurolemma into Xenopus laevis oocytes as a technique to study the effect of neurotoxicants on endogenous voltage-sensitive ion channels. Neurotoxicology 2017, 60, 260–273. [Google Scholar] [CrossRef]
  35. Miledi, R. A calcium-dependent transient outward current in Xenopus laevis oocytes. Proc. R. Soc. Lond. B. Biol. Sci. 1982, 215, 491–497. [Google Scholar] [CrossRef] [PubMed]
  36. Barish, M.E. A transient calcium-dependent chloride current in the immature Xenopus oocyte. J. Physiol. 1983, 342, 309–325. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  37. Browne, C.L.; Wiley, H.S.; Dumont, J.N. Oocyte-follicle cell gap junctions in Xenopus laevis and the effects of gonadotropin on their permeability. Science 1979, 203, 182–183. [Google Scholar] [CrossRef] [PubMed]
  38. Zhang, J.; Yuan, H.; Yao, X.; Chen, S. Endogenous ion channels expressed in human embryonic kidney (HEK-293) cells. Pflugers Arch.-Eur. J. Physiol. 2022, 474, 665–680. [Google Scholar] [CrossRef]
  39. Madeja, M.; Musshoff, U.; Speckmann, E.J. Follicular tissues reduce drug effects on ion channels in oocytes of Xenopus laevis. Eur. J. Neurosci. 1997, 9, 599–604. [Google Scholar] [CrossRef]
  40. Gielen, M.; Corringer, P.-J. The dual-gate model for pentameric ligand-gated ion channels activation and desensitization. J. Physiol. 2018, 596, 1873–1902. [Google Scholar] [CrossRef] [Green Version]
  41. Buller, A.L.; White, M.M. Altered patterns of N-linked glycosylation of the Torpedo acetylcholine receptor expressed in Xenopus oocytes. J. Membr. Biol. 1990, 115, 179–189. [Google Scholar] [CrossRef]
  42. Sivilotti, L.G.; McNeil, D.K.; Lewis, T.M.; Nassar, M.A.; Schoepfer, R.; Colquhoun, D. Recombinant nicotinic receptors, expressed in Xenopus oocytes, do not resemble native rat sympathetic ganglion receptors in single-channel behaviour. J. Physiol. 1997, 500, 123–138. [Google Scholar] [CrossRef]
  43. Truong, A.; Xing, X.; Forsayeth, J.R.; Dwoskin, L.P.; Crooks, P.A.; Cohen, B.N. Pharmacological differences between immunoisolated native brain and heterologously expressed rat alpha4beta2 nicotinic receptors. Brain Res. Mol. Brain Res. 2001, 96, 68–76. [Google Scholar] [CrossRef]
  44. Jospin, M.; Bonneau, B.; Lainé, V.; Bessereau, J.L. An extracellular scaffolding complex confers unusual rectification upon an ionotropic acetylcholine receptor in C. elegans. Proc. Natl. Acad. Sci. USA 2022, 119, e2113545119. [Google Scholar] [CrossRef]
  45. Opekarová, M.; Tanner, W. Specific lipid requirements of membrane proteins-a putative bottleneck in heterologous expression. Biochim. Biophys. Acta 2003, 1610, 11–22. [Google Scholar] [CrossRef] [Green Version]
  46. Mesoy, S.M.; Bridgland-Taylor, M.; Lummis, S.C.R. Mutations of the nACh Receptor M4 Helix Reveal Different Phenotypes in Different Expression Systems: Could Lipids be Responsible? Front. Physiol. 2022, 13, 850782. [Google Scholar] [CrossRef] [PubMed]
  47. Marsal, J.; Tigyi, G.; Miledi, R. Incorporation of acetylcholine receptors and Cl- channels in Xenopus oocytes injected with Torpedo electroplaque membranes. Proc. Natl. Acad. Sci. USA 1995, 92, 5224–5228. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  48. Bernareggi, A.; Reyes-Ruiz, J.M.; Lorenzon, P.; Ruzzier, F.; Miledi, R. Microtransplantation of acetylcholine receptors from normal or denervated rat skeletal muscles to frog oocytes. J. Physiol. 2011, 589, 1133–1142. [Google Scholar] [CrossRef]
  49. Palma, E.; Inghilleri, M.; Conti, L.; Deflorio, C.; Frasca, V.; Manteca, A.; Pichiorri, F.; Roseti, C.; Torchia, G.; Limatola, C.; et al. Physiological characterization of human muscle acetylcholine receptors from ALS patients. Proc. Natl. Acad. Sci. USA 2011, 108, 20184–20188. [Google Scholar] [CrossRef] [Green Version]
  50. Olivera-Bravo, S.; Ivorra, I.; Morales, A. Differential effects of quaternary ammonium anticholinesterases on microtransplanted neuroreceptors: Selective modulation of nicotinic receptor function. J. Mol. Neurosci. 2010, 40, 251–252. [Google Scholar] [CrossRef]
  51. Sanna, E.; Motzo, C.; Usala, M.; Pau, D.; Cagetti, E.; Biggio, G. Functional changes in rat nigral GABA(A) receptors induced by degeneration of the striatonigral GABAergic pathway: An electrophysiological study of receptors incorporated into Xenopus oocytes. J. Neurochem. 1998, 70, 2539–2544. [Google Scholar] [CrossRef]
  52. Miledi, R.; Eusebi, F.; Martínez-Torres, A.; Palma, E.; Trettel, F. Expression of functional neurotransmitter receptors in Xenopus oocytes after injection of human brain membranes. Proc. Natl. Acad. Sci. USA 2002, 99, 13238–13242. [Google Scholar] [CrossRef]
  53. Palma, E.; Torchia, G.; Limatola, C.; Trettel, F.; Arcella, A.; Cantore, G.; Di Gennaro, G.; Manfredi, M.; Esposito, V.; Quarato, P.P.; et al. BDNF modulates GABAA receptors microtransplanted from the human epileptic brain to Xenopus oocytes. Proc. Natl. Acad. Sci. USA 2005, 102, 1667–1672. [Google Scholar] [CrossRef] [Green Version]
  54. Palma, E.; Spinelli, G.; Torchia, G.; Martínez-Torres, A.; Ragozzino, D.; Miledi, R.; Eusebi, F. Abnormal GABAA receptors from the human epileptic hippocampal subiculum microtransplanted to Xenopus oocytes. Proc. Natl. Acad. Sci. USA. 2005, 102, 2514–2518. [Google Scholar] [CrossRef] [Green Version]
  55. Palma, E.; Amici, M.; Sobrero, F.; Spinelli, G.; Di Angelantonio, S.; Ragozzino, D.; Mascia, A.; Scoppetta, C.; Esposito, V.; Miledi, R.; et al. Anomalous levels of Cl- transporters in the hippocampal subiculum from temporal lobe epilepsy patients make GABA excitatory. Proc. Natl. Acad. Sci. USA 2006, 103, 8465–8468. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  56. Palma, E.; Roseti, C.; Maiolino, F.; Fucile, S.; Martinello, K.; Mazzuferi, M.; Aronica, E.; Manfredi, M.; Esposito, V.; Cantore, G.; et al. GABA(A)-current rundown of temporal lobe epilepsy is associated with repetitive activation of GABA(A) “phasic” receptors. Proc. Natl. Acad. Sci. USA 2007, 104, 20944–20948. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  57. Palma, E.; Ragozzino, D.; Di Angelantonio, S.; Mascia, A.; Maiolino, F.; Manfredi, M.; Cantore, G.; Esposito, V.; Di Gennaro, G.; Quarato, P.; et al. The antiepileptic drug levetiracetam stabilizes the human epileptic GABAA receptors upon repetitive activation. Epilepsia 2007, 48, 1842–1849. [Google Scholar] [CrossRef] [PubMed]
  58. Limon, A.; Reyes-Ruiz, J.M.; Miledi, R. Microtransplantation of neurotransmitter receptors from postmortem autistic brains to Xenopus oocytes. Proc. Natl. Acad. Sci. USA 2008, 105, 10973–10977. [Google Scholar] [CrossRef] [Green Version]
  59. Alberola-Die, A.; Fernández-Ballester, G.; González-Ros, J.M.; Ivorra, I.; Morales, A. Muscle-type nicotinic receptor blockade by diethylamine, the hydrophilic moiety of lidocaine. Front. Mol. Neurosci. 2016, 9, 12. [Google Scholar] [CrossRef] [Green Version]
  60. Alberola-Die, A.; Fernández-Ballester, G.; González-Ros, J.M.; Ivorra, I.; Morales, A. Muscle-type nicotinic receptor modulation by 2,6-dimethylaniline, a molecule resembling the hydrophobic moiety of lidocaine. Front. Mol. Neurosci. 2016, 9, 127. [Google Scholar] [CrossRef] [Green Version]
  61. Mazzo, F.; Zwart, R.; Serratto, G.M.; Gardinier, K.M.; Porter, W.; Reel, J.; Maraula, G.; Sher, E. Reconstitution of synaptic ion channels from rodent and human brain in Xenopus oocytes: A biochemical and electrophysiological characterization. J. Neurochem. 2016, 138, 384–396. [Google Scholar] [CrossRef] [Green Version]
  62. Burgos, J.S.; Aleu, J.; Barat, A.; Solsona, C.; Marsal, J.; Ramírez, G. Kainate-triggered currents in Xenopus oocytes injected with chick retinal membrane fragments: Effect of guanine nucleotides. Investig. Ophthalmol. Vis. Sci. 2003, 44, 3124–3129. [Google Scholar] [CrossRef]
  63. Bernareggi, A.; Dueñas, Z.; Reyes-Ruiz, J.M.; Ruzzier, F.; Miledi, R. Properties of glutamate receptors of Alzheimer’s disease brain transplanted to frog oocytes. Proc. Natl. Acad. Sci. USA 2007, 104, 2956–2960. [Google Scholar] [CrossRef] [Green Version]
  64. Sandoval, M.; Sandoval, R.; Thomas, U.; Spilker, C.; Smalla, K.H.; Falcon, R.; Marengo, J.J.; Calderón, R.; Saavedra, V.; Heumann, R.; et al. Antagonistic effects of TrkB and p75(NTR) on NMDA receptor currents in post-synaptic densities transplanted into Xenopus oocytes. J. Neurochem. 2007, 101, 1672–1684. [Google Scholar] [CrossRef] [PubMed]
  65. Miledi, R.; Dueñas, Z.; Martinez-Torres, A.; Kawas, C.H.; Eusebi, F. Microtransplantation of functional receptors and channels from the Alzheimer’s brain to frog oocytes. Proc. Natl. Acad. Sci. USA 2004, 101, 1760–1763. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Ivorra, I.; Henriquez, M.; Lax, P.; Riquelme, G.; Morales, A. Functional transplantation of chloride channels from the human syncytiotrophoblast microvillous membrane to Xenopus oocytes. Pflug. Arch.-Eur. J. Physiol. 2002, 444, 685–691. [Google Scholar] [CrossRef]
  67. Morales, A.; Aleu, J.; Ivorra, I.; Ferragut, J.A.; González-Ros, J.M.; Miledi, R. Incorporation of reconstituted acetylcholine receptors from Torpedo into the Xenopus oocyte membrane. Proc. Natl. Acad. Sci. USA 1995, 92, 8468–8472. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  68. Morales, A.; de Juan, E.; Fernández-Carvajal, A.M.; Martinez-Pinna, J.; Poveda, J.A.; Encinar, J.A.; Ivorra, I.; González-Ros, J.M. Nicotinic acetylcholine receptor properties are modulated by surrounding lipids: An in vivo study. J. Mol. Neurosci. 2006, 30, 5–6. [Google Scholar] [CrossRef] [Green Version]
  69. Le Cahérec, F.; Bron, P.; Verbavatz, J.M.; Garret, A.; Morel, G.; Cavalier, A.; Bonnec, G.; Thomas, D.; Gouranton, J.; Hubert, J.F. Incorporation of proteins into (Xenopus) oocytes by proteoliposome microinjection: Functional characterization of a novel aquaporin. J. Cell Sci. 1996, 109, 1285–1295. [Google Scholar] [CrossRef]
  70. Thompson, M.J.; Baenziger, J.E. Ion channels as lipid sensors: From structures to mechanisms. Nat. Chem. Biol. 2020, 16, 1331–1342. [Google Scholar] [CrossRef]
  71. Vallés, A.S.; Barrantes, F.J. Dysregulation of neuronal nicotinic acetylcholine receptor-cholesterol crosstalk in autism spectrum disorder. Front. Mol. Neurosci. 2021, 14, 744597. [Google Scholar] [CrossRef]
  72. Martinac, B.; Hamill, O.P. Gramicidin A channels switch between stretch activation and stretch inactivation depending on bilayer thickness. Proc. Natl. Acad. Sci. USA 2002, 99, 4308–4312. [Google Scholar] [CrossRef]
  73. Lundbaek, J.A.; Birn, P.; Hansen, A.J.; Søgaard, R.; Nielsen, C.; Girshman, J.; Bruno, M.J.; Tape, S.E.; Egebjerg, J.; Greathouse, D.V.; et al. Regulation of sodium channel function by bilayer elasticity: The importance of hydrophobic coupling. Effects of Micelle-forming amphiphiles and cholesterol. J. Gen. Physiol. 2004, 123, 599–621. [Google Scholar] [CrossRef] [Green Version]
  74. Gal, B.; Ivorra, I.; Morales, A. Functional incorporation of exogenous proteins into the Xenopus oocyte membrane does not depend on intracellular calcium increase. Pflug. Arch.-Eur. J. Physiol. 2000, 440, 852–857. [Google Scholar] [CrossRef]
  75. Tigyi, G.; Dyer, D.; Matute, C.; Miledi, R. A serum factor that activates the phosphatidylinositol phosphate signaling system in Xenopus oocytes. Proc. Natl. Acad. Sci. USA 1990, 87, 1521–1525. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  76. Durieux, M.E.; Salafranca, M.N.; Lynch, K.R.; Moorman, J.R. Lysophosphatidic acid induces a pertussis toxin-sensitive Ca(2+)-activated Cl- current in Xenopus laevis oocytes. Am. J. Physiol. 1992, 263, C896–C900. [Google Scholar] [CrossRef] [PubMed]
  77. Joardar, A.; Pattnaik, G.P.; Chakraborty, H. Mechanism of membrane fusion: Interplay of lipid and peptide. J. Membr. Biol. 2022, 255, 211–224. [Google Scholar] [CrossRef] [PubMed]
  78. Unwin, N. Protein-lipid interplay at the neuromuscular junction. Microscopy 2022, 71, i66–i71. [Google Scholar] [CrossRef]
  79. Unwin, N. Structure of a cholinergic cell membrane. Proc. Natl. Acad. Sci. USA 2022, 119, e2207641119. [Google Scholar] [CrossRef]
  80. Fong, T.M.; McNamee, M.G. Correlation between acetylcholine receptor function and structural properties of membranes. Biochemistry 1986, 25, 830–840. [Google Scholar] [CrossRef]
  81. Fernández-Ballester, G.; Castresana, J.; Fernández, A.M.; Arrondo, J.L.; Ferragut, J.A.; González-Ros, J.M. A role for cholesterol as a structural effector of the nicotinic acetylcholine receptor. Biochemistry 1994, 33, 4065–4071. [Google Scholar] [CrossRef]
  82. Fernández, A.M.; Poveda, J.A.; Encinar, J.A.; Morales, A.; González-Ros, J.M. Structural and functional modulation of ion channels by specific lipids: From model systems to cell membranes. In Protein-Lipid Interactions, 1st ed.; Mateo, C.R., Gómez, J., Villalaín, J., González-Ros, J.M., Eds.; Springer Series in Biophysics; Springer: Berlin, Germany, 2006; Volume 9, pp. 121–231. [Google Scholar] [CrossRef]
  83. Poveda, J.A.; Giudici, M.A.; Renart, L.M.; Morales, A.; González-Ros, J.M. Towards understanding the molecular basis of ion channel modulation by lipids: Mechanistic models and current paradigms. Biochim. Biophys. Acta Biomembr. 2017, 1859, 1507–1516. [Google Scholar] [CrossRef]
  84. daCosta, C.J.; Ogrel, A.A.; McCardy, E.A.; Blanton, M.P.; Baenziger, J.E. Lipid-protein interactions at the nicotinic acetylcholine receptor. A functional coupling between nicotinic receptors and phosphatidic acid-containing lipid bilayers. J. Biol. Chem. 2002, 277, 201–208. [Google Scholar] [CrossRef] [Green Version]
  85. Poveda, J.A.; Encinar, J.A.; Fernández, A.M.; Mateo, C.R.; Ferragut, J.A.; González-Ros, J.M. Segregation of phosphatidic acid-rich domains in reconstituted acetylcholine receptor membranes. Biochemistry 2002, 41, 12253–12262. [Google Scholar] [CrossRef]
  86. Caldironi, H.A.; Alonso, T.S. Lipidic characterization of full-grown amphibian oocytes and their plasma membrane-enriched fractions. Lipids 1996, 31, 651–656. [Google Scholar] [CrossRef] [PubMed]
  87. Stith, B.J.; Hall, J.; Ayres, P.; Waggoner, L.; Moore, J.D.; Shaw, W.A. Quantification of major classes of Xenopus phospholipids by high performance liquid chromatography with evaporative light scattering detection. J. Lipid. Res. 2000, 41, 1448–1454. [Google Scholar] [CrossRef]
  88. Unwin, N. Segregation of lipids near acetylcholine-receptor channels imaged by cryo-EM. IUCrJ 2017, 4, 393–399. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  89. Unwin, N. Protein-lipid architecture of a cholinergic postsynaptic membrane. IUCrJ 2020, 7, 852–859. [Google Scholar] [CrossRef]
  90. González-Ros, J.M.; Llanillo, M.; Paraschos, A.; Martinez-Carrión, M. Lipid environment of acetylcholine receptor from Torpedo Californica. Biochemistry 1982, 21, 3467–3474. [Google Scholar] [CrossRef]
  91. Criado, M.; Eibl, H.; Barrantes, F.J. Effects of lipids on acetylcholine receptor. Essential need of cholesterol for maintenance of agonist-induced state transitions in lipid vesicles. Biochemistry 1982, 21, 3622–3629. [Google Scholar] [CrossRef]
  92. Hamouda, A.K.; Sanghvi, M.; Sauls, D.; Machu, T.K.; Blanton, M.P. Assessing the lipid requirements of the Torpedo californica nicotinic acetylcholine receptor. Biochemistry 2006, 45, 4327–4337. [Google Scholar] [CrossRef]
  93. Brannigan, G.; Hénin, J.; Law, R.; Eckenhoff, R.; Klein, M.L. Embedded cholesterol in the nicotinic acetylcholine receptor. Proc. Natl. Acad. Sci. USA 2008, 105, 14418–14423. [Google Scholar] [CrossRef] [Green Version]
  94. Santiago, J.; Guzmán, G.R.; Rojas, L.V.; Marti, R.; Asmar-Rovira, G.A.; Santana, L.F.; McNamee, M.; Lasal-de-Dominicci, J.A. Probing the effects of membrane cholesterol in the Torpedo californica acetylcholine receptor and the novel lipid-exposed mutation alpha C418W in Xenopus oocytes. J. Biol. Chem. 2001, 276, 46523–46532. [Google Scholar] [CrossRef] [Green Version]
  95. Latorre, R.; Labarca, P.; Naranjo, D. Surface charge effects on ion conduction in ion channels. Methods Enzym. 1992, 207, 471–501. [Google Scholar] [CrossRef]
  96. Anzai, K.; Takano, C.; Tanaka, K.; Kirino, Y. Asymmetrical lipid charge changes the subconducting state of the potassium channel from sarcoplasmic reticulum. Biochem. Biophys. Res. Commun. 1994, 199, 1081–1087. [Google Scholar] [CrossRef] [PubMed]
  97. Wrigglesworth, J.M.; Wooster, M.S.; Elsden, J.; Danneel, H.J. Dynamics of proteoliposome formation. Intermediate states during detergent dialysis. Biochem. J. 1987, 246, 737–744. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  98. Richards, M.J.; Hsia, C.Y.; Singh, R.R.; Haider, H.; Kumpf, J.; Kawate, T.; Daniel, S. Membrane protein mobility and orientation preserved in supported bilayers created directly from cell plasma membrane blebs. Langmuir 2016, 32, 2963–2974. [Google Scholar] [CrossRef] [PubMed]
  99. Vitrac, H.; MacLean, D.M.; Jayaraman, V.; Bogdanov, M.; Dowhan, W. Dynamic membrane protein topological switching upon changes in phospholipid environment. Proc. Natl. Acad. Sci. USA 2015, 112, 13874–13879. [Google Scholar] [CrossRef] [Green Version]
  100. Pace, H.; Simonsson Nyström, L.; Gunnarsson, A.; Eck, E.; Monson, C.; Geschwindner, S.; Snijder, A.; Höök, F. Preserved transmembrane protein mobility in polymer-supported lipid bilayers derived from cell membranes. Anal. Chem. 2015, 87, 9194–9203. [Google Scholar] [CrossRef]
  101. Stockbridge, R.B.; Tsai, M.F. Lipid reconstitution and recording of recombinant ion channels. Methods Enzym. 2015, 556, 385–404. [Google Scholar] [CrossRef]
  102. Sejwal, K.; Chami, M.; Baumgartner, P.; Kowal, J.; Müller, S.; Stahlberg, H. Proteoliposomes-a system to study membrane proteins under buffer gradients by cryo-EM. Nanotechnol. Rev. 2017, 6, 57–74. [Google Scholar] [CrossRef]
  103. Poveda, J.A.; Giudici, A.M.; Renart, M.L.; Millet, O.; Morales, A.; González-Ros, J.M.; Oakes, V.; Furini, S.; Domene, C. Modulation of the potassium channel KcsA by anionic phospholipids: Role of arginines at the non-annular lipid binding sites. Biochim. Biophys. Acta Biomembr. 2019, 1861, 183029. [Google Scholar] [CrossRef]
  104. Renart, M.L.; Giudici, A.M.; Díaz-García, C.; Molina, M.L.; Morales, A.; González-Ros, J.M.; Poveda, J.A. Modulation of function, structure and clustering of K+ channels by lipids: Lessons learnt from KcsA. Int. J. Mol. Sci. 2020, 21, 2554. [Google Scholar] [CrossRef] [Green Version]
  105. Olivera-Bravo, S.; Ivorra, I.; Morales, A. The acetylcholinesterase inhibitor BW284c51 is a potent blocker of Torpedo nicotinic AchRs incorporated into the Xenopus oocyte membrane. Br. J. Pharmacol. 2005, 144, 88–97. [Google Scholar] [CrossRef] [Green Version]
  106. Olivera-Bravo, S.; Ivorra, I.; Morales, A. Diverse inhibitory actions of quaternary ammonium cholinesterase inhibitors on Torpedo nicotinic ACh receptors transplanted to Xenopus oocytes. Br. J. Pharmacol. 2007, 151, 1280–1292. [Google Scholar] [CrossRef] [PubMed]
  107. Alberola-Die, A.; Martinez-Pinna, J.; González-Ros, J.M.; Ivorra, I.; Morales, A. Multiple inhibitory actions of lidocaine on Torpedo nicotinic acetylcholine receptors transplanted to Xenopus oocytes. J. Neurochem. 2011, 117, 1009–1019. [Google Scholar] [CrossRef]
  108. Cobo, R.; Nikolaeva, M.; Alberola-Die, A.; Fernández-Ballester, G.; González-Ros, J.M.; Ivorra, I.; Morales, A. Mechanisms underlying the strong inhibition of muscle-type nicotinic receptors by tetracaine. Front. Mol. Neurosci. 2018, 11, 193. [Google Scholar] [CrossRef] [PubMed]
  109. Cobo, R.; Nikolaeva-Koleva, M.; Alberola-Die, A.; Fernández-Ballester, G.; González-Ros, J.M.; Ivorra, I.; Morales, A. Mechanisms of blockade of the muscle-type nicotinic receptor by benzocaine, a permanently uncharged local anesthetic. Neuroscience 2020, 439, 62–79. [Google Scholar] [CrossRef] [PubMed]
  110. Alberola-Die, A.; Encinar, J.A.; Cobo, R.; Fernández-Ballester, G.; González-Ros, J.M.; Ivorra, I.; Morales, A. Peimine, an anti-inflammatory compound from Chinese herbal extracts, modulates muscle-type nicotinic receptors. Int. J. Mol. Sci. 2021, 22, 11287. [Google Scholar] [CrossRef] [PubMed]
  111. Woodhull, A.M. Ionic blockage of sodium channels in nerve. J. Gen. Physiol. 1973, 61, 687–708. [Google Scholar] [CrossRef] [Green Version]
  112. Spitzer, N.C. A Rosetta stone for analysis of human membrane protein function. Proc. Natl. Acad. Sci. USA 2008, 105, 10641–10642. [Google Scholar] [CrossRef]
Membranes 12 00986 g001 550
Figure 1. Micrographs of Xenopus oocytes. (A) Image of an opened and extended fragment of the Xenopus ovary lobule, showing oocytes at different stages of development. (B) Full-grown, immature oocyte, and the plasma membrane (together with its vitelline envelope) from another oocyte, manually isolated and stained with ink for better observation.
Figure 1. Micrographs of Xenopus oocytes. (A) Image of an opened and extended fragment of the Xenopus ovary lobule, showing oocytes at different stages of development. (B) Full-grown, immature oocyte, and the plasma membrane (together with its vitelline envelope) from another oocyte, manually isolated and stained with ink for better observation.
Membranes 12 00986 g001
Membranes 12 00986 g002 550
Figure 2. Methodology followed to microtransplant foreign membrane proteins to oocytes. Scheme of the steps to microtransplant the purified and reconstituted nicotinic acetylcholine (ACh) receptors (nAChRs) to the Xenopus oocyte membrane to carry out detailed functional studies.
Figure 2. Methodology followed to microtransplant foreign membrane proteins to oocytes. Scheme of the steps to microtransplant the purified and reconstituted nicotinic acetylcholine (ACh) receptors (nAChRs) to the Xenopus oocyte membrane to carry out detailed functional studies.
Membranes 12 00986 g002
Membranes 12 00986 g003 550
Figure 3. The microtransplantation of proteoliposomes to the Xenopus oocyte membrane does not depend on the increase in the intracellular calcium concentration ([Ca2+]i). ACh-elicited currents in oocytes microinjected with proteolipomes bearing nAChRs in the control oocytes (left, control) and in oocytes previously loaded with ca. 5 nM EGTA to chelate [Ca2+]i (right). Note the slower desensitization on nAChRs in the EGTA loaded cell.
Figure 3. The microtransplantation of proteoliposomes to the Xenopus oocyte membrane does not depend on the increase in the intracellular calcium concentration ([Ca2+]i). ACh-elicited currents in oocytes microinjected with proteolipomes bearing nAChRs in the control oocytes (left, control) and in oocytes previously loaded with ca. 5 nM EGTA to chelate [Ca2+]i (right). Note the slower desensitization on nAChRs in the EGTA loaded cell.
Membranes 12 00986 g003
Membranes 12 00986 g004 550
Figure 4. Patchy distribution of microtransplanted nAChRs on the oocyte surface. (A) Scheme showing patches of microtransplanted nAChRs on the oocyte surface (red spots) to be activated by the ACh solution superfused from a nearby tube. (B) Two superimposed IAChs showing at least two sizeable “humps” (more evident in the derivatives of IACh records shown below), which were most likely due to the subsequent activation of large patches of nAChRs.
Figure 4. Patchy distribution of microtransplanted nAChRs on the oocyte surface. (A) Scheme showing patches of microtransplanted nAChRs on the oocyte surface (red spots) to be activated by the ACh solution superfused from a nearby tube. (B) Two superimposed IAChs showing at least two sizeable “humps” (more evident in the derivatives of IACh records shown below), which were most likely due to the subsequent activation of large patches of nAChRs.
Membranes 12 00986 g004
Membranes 12 00986 g005 550
Figure 5. Protein function depends on its adequate orientation in the membrane after microtransplantation. (A) Scheme of the putative orientation in the plasma membrane of the microtransplanted nAChRs after intracellular injection of proteoliposomes bearing this protein. Note that the orientation of nAChRs in the injected proteoliposomes was mostly outside-out (left; ACh-binding sites shown as green spheres), whereas it turned to the outside-in orientation after the proteoliposome fused with the plasma membrane (right-side panel). nAChRs adopting a “wrong” orientation have been crossed out; Ec and Ic indicate extracellular and intracellular sides of the membrane, respectively. (B) nAChRs with an outside-in orientation lack functional activity, as evidenced by the lack of response when ACh was injected intracellularly (right panel). In contrast, focal ACh pulses over the oocyte surface, applied to nAChRs with the outside-out orientation, elicited IAChs (left).
Figure 5. Protein function depends on its adequate orientation in the membrane after microtransplantation. (A) Scheme of the putative orientation in the plasma membrane of the microtransplanted nAChRs after intracellular injection of proteoliposomes bearing this protein. Note that the orientation of nAChRs in the injected proteoliposomes was mostly outside-out (left; ACh-binding sites shown as green spheres), whereas it turned to the outside-in orientation after the proteoliposome fused with the plasma membrane (right-side panel). nAChRs adopting a “wrong” orientation have been crossed out; Ec and Ic indicate extracellular and intracellular sides of the membrane, respectively. (B) nAChRs with an outside-in orientation lack functional activity, as evidenced by the lack of response when ACh was injected intracellularly (right panel). In contrast, focal ACh pulses over the oocyte surface, applied to nAChRs with the outside-out orientation, elicited IAChs (left).
Membranes 12 00986 g005
Membranes 12 00986 g006 550
Figure 6. Modulation of nAChR function by specific lipids. (A) IAChs elicited in oocytes injected with proteoliposomes bearing nAChRs reconstituted in either asolectin (R-Aso), phosphatidylcholine (PC) and Chol (R-PC+Chol), or phosphatidic acid (PA), PC, and Chol (R-PA+PC+Chol). Notice the larger IACh in the R-PA+PC+Chol oocyte. (B) Effect of pre-injecting the oocyte with liposomes of different composition (Aso, PA, or PA+PC+Chol) 6 h before microinjecting proteoliposomes bearing nAChRs reconstituted in Aso (R-Aso). Left, the scheme shows the experimental procedure. Right, column bars comparing the relative amplitude of the IAChs of the indicated groups with respect to the control values (in oocytes pre-injected with Aso liposomes).
Figure 6. Modulation of nAChR function by specific lipids. (A) IAChs elicited in oocytes injected with proteoliposomes bearing nAChRs reconstituted in either asolectin (R-Aso), phosphatidylcholine (PC) and Chol (R-PC+Chol), or phosphatidic acid (PA), PC, and Chol (R-PA+PC+Chol). Notice the larger IACh in the R-PA+PC+Chol oocyte. (B) Effect of pre-injecting the oocyte with liposomes of different composition (Aso, PA, or PA+PC+Chol) 6 h before microinjecting proteoliposomes bearing nAChRs reconstituted in Aso (R-Aso). Left, the scheme shows the experimental procedure. Right, column bars comparing the relative amplitude of the IAChs of the indicated groups with respect to the control values (in oocytes pre-injected with Aso liposomes).
Membranes 12 00986 g006
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Ivorra, I.; Alberola-Die, A.; Cobo, R.; González-Ros, J.M.; Morales, A. Xenopus Oocytes as a Powerful Cellular Model to Study Foreign Fully-Processed Membrane Proteins. Membranes 2022, 12, 986. https://doi.org/10.3390/membranes12100986

AMA Style

Ivorra I, Alberola-Die A, Cobo R, González-Ros JM, Morales A. Xenopus Oocytes as a Powerful Cellular Model to Study Foreign Fully-Processed Membrane Proteins. Membranes. 2022; 12(10):986. https://doi.org/10.3390/membranes12100986

Chicago/Turabian Style

Ivorra, Isabel, Armando Alberola-Die, Raúl Cobo, José Manuel González-Ros, and Andrés Morales. 2022. "Xenopus Oocytes as a Powerful Cellular Model to Study Foreign Fully-Processed Membrane Proteins" Membranes 12, no. 10: 986. https://doi.org/10.3390/membranes12100986

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop