Open Access

Tuning microbial hosts for membrane protein production

Microbial Cell Factories20098:69

DOI: 10.1186/1475-2859-8-69

Received: 15 October 2009

Accepted: 29 December 2009

Published: 29 December 2009


The last four years have brought exciting progress in membrane protein research. Finally those many efforts that have been put into expression of eukaryotic membrane proteins are coming to fruition and enable to solve an ever-growing number of high resolution structures. In the past, many skilful optimization steps were required to achieve sufficient expression of functional membrane proteins. Optimization was performed individually for every membrane protein, but provided insight about commonly encountered bottlenecks and, more importantly, general guidelines how to alleviate cellular limitations during microbial membrane protein expression. Lately, system-wide analyses are emerging as powerful means to decipher cellular bottlenecks during heterologous protein production and their use in microbial membrane protein expression has grown in popularity during the past months.

This review covers the most prominent solutions and pitfalls in expression of eukaryotic membrane proteins using microbial hosts (prokaryotes, yeasts), highlights skilful applications of our basic understanding to improve membrane protein production. Omics technologies provide new concepts to engineer microbial hosts for membrane protein production.


We have seen amazing advances in the field of membrane protein research over the past four years. For the first time, high resolution structures for pharmaceutically relevant eukaryotic membrane proteins, including class A G-protein coupled receptors (GPCR) [15], transporters [6] and channel proteins [716] became available and provided valuable insight into their mode of action (Table 1). A few years earlier, structures of the soluble domains of human CYP3A4 and CYP2D6 of the Cytochrome P450 family, the most important drug metabolising enzymes, had been solved [1720]. Actually, many years of strenuous efforts were required to get the proteins to crystals, relying on iterative optimization of all steps from expression to purification and crystallization. The total number of membrane protein structures deposited in the protein data bank (PDB) also strikingly reflects that membrane protein research can not yet keep pace with the one of soluble proteins. Among over 58,000 total entries, only some 100 of all coordinate sets belong to membrane proteins [21]. Nature, however, provides plenty of different targets: roughly one third of all open reading frames encode for membrane proteins, as predicted for fully sequenced genomes of eubacterial, archaean and eukaryotic organisms [22, 23]. The discrepancy between biodiversity and poor structural knowledge can be largely attributed to the low natural expression of membrane proteins, to their hydrophobic character which complicates overexpression of functional membrane proteins, as well as to difficulties during their purification and crystallization.
Table 1

Eukaryotic membrane proteins with high resolution structures.


Expression Host

PDB coordinates

Resolution (Å)



Beta-Barrel Membrane Proteins: Mitochondrial Outer Membrane

Human VDAC-1 voltage dependent anion channel

E. coli

2K4T1, 2JK42


[210, 211]

Murine VDAC-1 voltage dependent anion channel

E. coli





G Protein-Coupled Receptors

Rhodopsin: Bovine Rod Outer Segment mutant N2C/D282C

COS cells




Engineered turkey β1 adrenergic receptor

Trichoplusia ni




Human β2 adrenergic receptor, from β2AR365-Fab5 (2R4R) and β2AR24/365- Fab5 complexes (2R4S)

Spodoptera frugiperda

2R4R, 2R4S



Engineered human β2 adrenergic receptor

Spodoptera frugiperda

2RH1, 3D4S


[3, 4]

Human A2A adenosine receptor, In complex with a high-affinity subtype-selective antagonist ZM241385.

Spodoptera frugiperda




Integrin Adhesion Receptors

Human Integrin αIIbβ3 transmembrane-cytoplasmic heterodimer, NMR Structure

E. coli




Snare Protein Family

Syntaxin 1A/SNAP-25/Synaptobrevin-2 Complex from Rattus rattus

E. coli




Ion Channels

Kir3.1-Prokaryotic Kir Chimera: Mus musculus & Burkholderia xenovorans

E. coli




ASIC1 Acid-Sensing Ion Channel: Gallus gallus; 2QTS: N- and C-terminal deletions, 3HGC: minimal functional channel

Spodoptera frugiperda



[8, 215]

ATP-gated P2X4 ion channel (apo protein): Danio rerio (zebra fish) (expressed in SF9 cells), 3.1 Å; Closed state. A construct, 3.5 Å: 3I5D

Spodoptera frugiperda

3H9V, 3I5D



Kv1.2 Voltage-gated potassium Channel: Rattus norvegicus

Pichia pastoris




Kv1.2/Kv2.1 Voltage-gated potassium channel chimera: Rattus norvegicus

Pichia pastoris




Other Channels: Aquaporins and Glyceroporins

Rat AQP4 aquaporin water channel, S180D mutant (2ZZ9)

Spodoptera frugiperda

2D57, 2ZZ9


[11, 12]

Human AQP4 aquaporin water channel

Pichia pastoris




Human AQP5 aquaporin water channel

Pichia pastoris




Plant SoPIP2;1 aquaporin: Spinacia oleracea in closed (1Z98) and open conformation (2B5F)

Pichia pastoris

1Z98, 2B5F



Pichia pastoris AQY1 aquaporin, pH 3.5 (2W2E) and 8.0 (2W1P)

Pichia pastoris

2W2E, 2W1P



Other Channels: Gap Junctions

Human Connexin 26 (Cx26; GJB2) gap junction

Spodoptera frugiperda




Membrane-Associated Proteins in Eicosanoid and Glutathione Metabolism

Human Microsomal Prostaglandin E Synthase 1: Human (Electron Diffraction) In complex with glutathione.

E. coli




Human 5-Lipoxygenase-Activating Protein (FLAP) with Bound MK-591 Inhibitor (2Q7M), FLAP with iodinated MK-591 analog (2Q7R)

E. coli

2Q7M, 2Q7R



Human Leukotriene LTC4 Synthase in complex with glutathione

S. pombe




Human Leukotriene LTC4 Synthase in complex with glutathione/apo form

Pichia pastoris




ATP Binding Cassette Transporters

Mus musculus P-Glycoprotein (3G5U), With bound QZ59-RRR (3G60) and QZ59-SSS (3G61)

Pichia pastoris

3G5U, 3G60, 3G61



P-type ATPase

Human Na,K-ATPase Regulatory Protein FXYD1

E. coli




Phospholamban homopentamer: Human sarcoplasmic reticulum

E. coli

1ZLL1, 1FJK1, 1FJP1



Plasma Membrane H+-ATPase: Arabidopsis thaliana

S. cerevisiae




1 Structure determined by NMR spectroscopy,

2 Structure determined by combining X-ray and NMR data.

Paradoxically, from a pharmaceutical point of view, membrane proteins - in particular GPCRs and transport proteins - constitute key drug targets, as most signal transduction processes are initiated or transmitted via membrane proteins. The facts that at least 50% of all commercially available drugs target membrane proteins, that the major enzymes initiating drug metabolism are microsomal cytochrome P450 enzymes and that the human immune defense against invading pathogens is often initiated by their membrane proteins [24, 25], underline the importance of elucidating three-dimensional structures of membrane proteins [26]. Evidently, great efforts are made to better understand membrane proteins from a structural and functional point of view. Unfortunately, (recombinant) expression of eukaryotic membrane proteins often suffered from low expression levels, instability of proteins and/or degradation by the host's proteolytic machinery. While in the past many labs have focused on their single targets, there was a strong trend towards studying a large number of different proteins simultaneously more recently. In this regard, many consortia and research groups have tried to rationalize all processes from expression to purification and crystallization, hoping to end up with at least a few membrane proteins that are amenable to crystallization (structural genomics). Whatever route is taken, it is obvious that improvements in early steps, particularly concerning expression levels of functional membrane proteins are of tremendous benefit to subsequent experiments, especially protein purification, characterization and crystallization.


1. Expression systems

In the past, unreasonably more structures have been solved for bacterial and archaebacterial membrane proteins than for eukaryotic ones (Database of Membrane Proteins of Known Structure [21]). Early success in crystallization of eukaryotic membrane proteins came from the use of native proteins [2731]. However, this was only successful if a uniquely rich source was available, e.g. the retina providing mg amounts of rhodopsin, and it precluded protein modifications, e.g. isotope labelling for NMR analysis. Due to difficulties in isolating native membrane proteins in sufficient quantity and quality, strong efforts were made towards establishing heterologous expression systems for the production of eukaryotic membrane proteins. Prior to 2005, no high resolution structure had been solved for any recombinant eukaryotic membrane protein. Since then, 28 unique structures have been elucidated for eukaryotic membrane proteins (Table 1). Among microbes, the prokaryote E. coli and the yeast Pichia pastoris have been most successfully used in production of eukaryotic membrane proteins for structural analyses.

1.1. Prokaryotic expression systems and their limitations in hosting eukaryotic membrane proteins

E. coli still tops the list of the most popular expression systems for prokaryotic and eukaryotic membrane proteins, given the broad choice of molecular biology tools and strains available [32]. Its ease of handling, especially in a high-throughput way, enabling analyses of many proteins in parallel, sophisticated genetic manipulation techniques, the availability of membrane protein-adapted strains, but also cost effectiveness - all these factors contribute to the popularity of E. coli and its preferential use in structural genomics initiatives targeting membrane proteins of both prokaryotic and eukaryotic origin. While E. coli provides an optimal environment for prokaryotic proteins, its capability to host eukaryotic membrane proteins was limited, however [26, 33]. Although reasonable success in providing eukaryotic membrane proteins for structural analyses has been documented (Table 1), success rates are low compared to eukaryotic expression hosts. Often, prokaryotic homologues are studied in lieu of eukaryotic membrane proteins. However, only 13% of all membrane protein families are common between prokaryotes and eukaryotes [34].

For eukaryotic proteins, prokaryotic folding pathways might be far from optimal, as subtle differences between assembly machineries impede their correct processing. While the eukaryotic translocon possesses charged residues mediating interaction with the nascent polypeptide chain during translocation and insertion into the membrane, bacterial counterparts are lacking these features [35]. Additionally, the membrane composition of different eukaryotic organellar membranes is different from the prokaryotic cytoplasmic membrane and also processing of premature proteins often fails in prokaryotes, likely leading to mistargeting or misfolding of eukaryotic membrane proteins [36]. Apart from incompatibilities in protein processing, varying polypeptide elongation and folding rates contribute to the obstacles experienced in heterologous expression of eukaryotic membrane proteins in prokaryotic hosts [37]. The rate of polypeptide chain elongation is 4 to 10 times faster in prokaryotes compared to eukaryotic cells. As all steps during translation, folding and membrane insertion need to be properly balanced allowing the protein to find its native conformation, high translation rates might lead to exposure of hydrophobic segments, and thus promote their aggregation. In the past, membrane protein expression was performed just like expression of simple soluble proteins. Strong promoter systems have been preferentially employed to drive expression, e.g. T7 promoter, thereby obviously exceeding the translocation machinery's ability to correctly process the enzyme [38]. As a consequence of high transcript abundance combined with high prokaryotic translational rates, eukaryotic membrane proteins often accumulate in inclusion bodies [26, 39]. At first view, this offers some apparent advantages such as no or reduced toxicity caused by heterologously expressed proteins, protection against proteases and, thus, high yields. However, inclusion bodies require renaturation, which is anything but trivial. Although some membrane proteins have been successfully refolded from inclusion bodies [40], in vitro renaturation remains a contentious issue, as many proteins fail in reaching the native, functional conformation once they are denatured. Refolding has been most successfully employed for β-barrel type membrane proteins, which are innately more robust than α-helical membrane proteins, but also not as sought after as the latter [41]. Therefore, expression of properly folded and membrane-embedded proteins is highly desirable, be it by attenuating expression strength, e.g. by the use of weak promoters and low copy number, be it by modifying cultivation conditions, e.g. growth temperature and inducer concentration, as will be discussed further below [38, 42]. In the case of low temperature, the effect of reduced transcription and translation rates seems to combine with the availability of additional chaperones and foldases [43].

Overexpression of eukaryotic proteins is furthermore often complicated due to E. coli's inability to perform posttranslational modifications that can be crucial for proper folding, targeting and function [44]. Many eukaryotic membrane proteins rely on the presence of specific post-translational modifications (PTM) to attain full activity, e.g. acylation and phosphorylation, or to retain stability mainly by glycosylation [33]. E. coli is not able to glycosylate proteins and, thus, not the host of choice if such modification is crucial for activity [33, 44, 45]. On the other hand, non-glycosylated proteins are usually rather homogeneous and uniform, which might be advantageous for experiments depending on very pure enzymes, e.g. crystallization. Often, phosphorylation events are necessary for protein activation e.g. triggering conformation changes as observed for many GPCRs, thus precluding in vivo studies [46, 47]. Further, E. coli lacks endogenous G proteins impeding its use for functional studies of GPCRs, but coexpression [48] or even external addition of the G protein α subunit to the membrane preparation was able to restore high-affinity binding properties [49].

According to the current view, membrane proteins exist as protein-lipid complexes with specific lipids inevitably required to promote folding, retain activity and confer structural stability, as can be seen from their presence in many crystal structures [36, 50, 51]. Bacterial membranes are devoid of sterols and derivatives, polyunsaturated fatty acid chains and sphingolipids, which are known to play a key role in folding of membrane proteins in eukaryotic membranes (reviewed in [36]). Failure to produce functional mammalian receptors in E. coli has thus been partly ascribed to the lack of essential lipids, e.g. cholesterol during expression of mammalian serotonin transporter [52, 53]. Many mitochondrial membrane proteins tightly interact with cardiolipin, and large amounts of F1F0 ATP synthase were only obtained after modulating lipid biosynthesis pathways and, thus, lipid composition of E. coli membranes towards an increased cardiolipin content [54]. In a few cases, the addition of lipids during expression and purification restored protein activity [36].

Although reasonable expression levels have been demonstrated for different individual eukaryotic membrane proteins [42], the most successful attempts have been found for β-barrel type membrane proteins (Table 1). Expression levels were typically several orders of magnitude lower compared to their bacterial homologs [52].

Besides E. coli, the gram-positive bacterium Lactococcus lactis has emerged as alternative prokaryotic host due to a relatively small number of endogenous membrane proteins and thus high capacity to host foreign proteins [5558]. As facultative anaerobic bacterium, L. lactis is able to reach high cell densities even under anaerobic conditions. Being surrounded by a single membrane, L. lactis cells can be broken easily, thereby facilitating downstream processes. Due to the relatively small genome i.e. approx. 50% of E. coli, however, some auxiliary proteins and chaperones with essential functions in folding and membrane insertion might not be provided by L. lactis [57]. While 21 of 25 (84%) prokaryotic transport proteins were successfully expressed in E. coli, only 10 thereof (40%) could be obtained in L. lactis cells, as demonstrated recently [59]. On the other hand, the proportion of functional protein of prokaryotic origin was higher in L. lactis compared to E. coli [60]. Though levels of eukaryotic membrane proteins lag still behind those obtained for prokaryotic ones, yields are comparable to those obtained in E. coli [57]. In light of the fact that formation of inclusion bodies has not been observed so far during expression of membrane proteins, L. lactis provides an attractive alternative to E. coli [55, 57].

The halophilic archaeon Halobacterium salinarum also ranges among promising non-standard expression hosts due to its elaborate membrane system and, thus, its high capacity to host additional membrane proteins. Nonetheless, high level expression seemed to be limited to bacteriorhodopsin and derivatives [61, 62]. Among prokaryotic hosts, the photosynthetic bacteria Rhodobacter sphaeroides and Rhodobacter capsulatus provide plenty of membrane space while concomitantly offering elaborate and highly efficient insertion machineries. During prototrophic growth, they use light for energy production and growth, and thereby enrich intracytoplasmic membranes [6365]. However future experiments will have to demonstrate whether this is sufficient to obtain high yields of membrane proteins.

1.2. Yeasts as expression systems for eukaryotic membrane proteins

Despite individual breakthroughs, prokaryotic expression systems tend to provide an inhospitable environment for eukaryotic membrane proteins. Therefore, most recent attempts were directed towards employing eukaryotic hosts for eukaryotic membrane protein expression. In this context, yeasts are an inexpensive, yet efficient alternative to prokaryotes. Providing a eukaryotic environment, yeast cells are capable of processing proteins similarly to higher eukaryotes. Simple handling, rapid growth and powerful genetic tools contributed to their popularity [66]. To date, 10 out of 28 unique structures of heterologously expressed eukaryotic membrane proteins were obtained from yeast-derived material, including the best-resolved structures (1.8 - 2.0 Å) of mammalian membrane proteins (Table 1) [13, 14, 67].

Most commonly, membrane proteins are overexpressed and targeted to the ER membrane from where they are transported to the plasma membrane in vesicles [68]. Unlike E. coli, yeasts are able to perform various post-translational modifications including proteolytic processing of signal sequences of both pre- and prepro-type, disulfide-bond formation, acylation, prenylation, phosphorylation and certain types of O- and N-linked glycosylation that all might be essential for activity and correct folding (reviewed in [66]). Methylotrophic yeasts are an attractive alternative to S. cerevisiae as overexpressed proteins are less frequently hyper-mannosylated than in S. cerevisiae. In addition, the presence of a terminal α-1,2-mannose residue abolishes their allergenic potential [69, 70]. Meanwhile, even strains with a more uniform and also with a human glycosylation pattern are available for functional studies [7174]. Although the lipid composition of yeast membranes is closer to higher eukaryotes than to E. coli, the lack of certain lipids, in particular sterols, e.g. cholesterol for mammalian proteins, sito-, stigma- and campesterol for plant enzymes, might affect protein functionality. Ergosterol, the predominant endogenous sterol in fungi, might compensate for specific sterols, as shown for mammalian GPCRs and transport proteins, but for full activity presence of cholesterol might be essential [33, 75]. During purification, protein activity and stability can be retained or even restored by addition of defined lipids. In this respect, cholesterol hemisuccinate was crucial in stabilizing the A2a receptor during purification following overexpression in S. cerevisiae [76].

Being the model eukaryote, S. cerevisiae has traditionally been most widely employed for the expression of eukaryotic membrane proteins [7779]. This popularity can be largely ascribed to elaborate, yet easy genetic manipulation techniques, as documented by the availability of numerous expression plasmids. Furthermore, the vast number of available strains including entire deletion libraries allows to carry out functional complementation in vivo, as exemplified recently for different plant transporter proteins [8082]. Most frequently, inducible promoters (e.g. GAL1 or GAL10) are employed to tune membrane protein expression by yeast as for 93% of membrane proteins constitutive expression resulted in impaired growth during their homologous overexpression [83, 84]. In contrast to other yeasts, protocols have been established for S. cerevisiae to enable its use in high-throughput (HTP)-expression studies of eukaryotic membrane proteins [7779]. While on the one hand a C-terminal GFP-His8-fusion is employed to assess expression levels and optimize purification [77, 78], other methods rely on the combination of C-terminal His10- and N-terminal FLAG-tags [79], using immunodetection for estimation of expression levels. Most commonly, episomal plasmids were used for expression. Ability of S. cerevisiae to perform in vivo recombination allows ligation of the respective gene into the expression plasmid in vivo [7779]. Additionally, in vivo cloning permits the simple construction of protein variants, as shown recently for mouse-TRPM5 channel [85], and, therefore, directed evolution of membrane proteins or selected domains.

Due to its tendency to hypermannosylate proteins and complex handling of S. cerevisiae in fermenter cultures, much attention has recently focused on non-conventional yeasts including Schizosaccharomyces pombe, Yarrowia lipolytica, Hansenula polymorpha and Pichia pastoris.

The fission yeast Schizosaccharomyces pombe outperforms other yeast species in expressing mammalian proteins with mammalian-like core glycosylation pattern and by its ability to process intron-containing genes [86, 87]. Thus, S. pombe is a promising, yet easy-to-handle alternative to conventional yeast species with a high potential for the expression of complex proteins, e.g GPCRs [88]. S. pombe's suitability to express functional eukaryotic membrane proteins was supported by a previous study on human D2S dopamine receptor, resulting in a five fold higher binding affinity of isolated membranes and, thus, a higher proportion of functional, membrane-integrated receptor compared to the protein produced in S. cerevisiae [89].

Frequently, heterologous systems are used for membrane protein expression to obtain sufficient amounts of those proteins for structural and functional studies in vitro. Apart from purification-oriented purposes, eukaryotic membrane proteins such as enzymes of the cytochrome P450 family are also overexpressed in heterologous systems to perform whole-cell biotransformations on highly valuable substances (reviewed in [90]). While initially bioconversions had been realized using S. cerevisiae [9197], meanwhile also S. pombe has been successfully employed for mammalian cytochrome P450-mediated reactions [98102]. As P450s act in concert with an electron-donating system, coupling efficiency and thus substrate conversion rates can be increased by coexpression of the respective mammalian redox partners or by protein engineering of the biocatalyst [103]. The origin and the quantity of the coexpressed reductase may influence the expression of the heme domain and the resulting activity of these complex enzymes. This is usually regulated by gene copy numbers or by the choice of the employed promoters.

Similarly, another non-conventional yeast species, Yarrowia lipolytica, is emerging as host for biotransformations of hydrophobic substrates as it tolerates organic solvents and metabolizes aliphatic compounds. Y. lipolytica has been employed for production of cytochrome P450 enzymes, including bovine P450 17α (CYP17A) [104], human P450 CYP1A1 [105] and CYP53B1 from Rhodotorula minuta [106]. From these studies evidence emerged that integration of multiple expression cassettes had a positive effect on heterologous expression as observed by increased conversion rates.

Among non-Saccharomyces yeasts, the methylotrophic yeast Pichia pastoris has been most extensively and successfully employed in membrane protein research (Table 1). Exceptionally high cell densities can be reached during cultivation, concomitantly guaranteeing efficient and economically sustainable protein production (reviewed in [107, 108]). Methylotrophic yeasts may derive all energy for growth from the utilization of methanol as carbon source by inducing expression of methanol-metabolizing enzymes, namely alcohol oxidase (AOX) and dihydroxyacetone synthase (DHAS) [109]. Because promoters of the methanol utilization pathway are strong but also tightly regulated, these are most commonly employed to drive heterologous protein expression [110, 111], allowing to reach up to 90 mg L-1 of membrane proteins exemplified by a human aquaporin [112]. Furthermore, protein production capacity is not compromised during growth on minimal media, which makes this yeast attractive for the production of stable isotope labelled proteins for NMR-based structural biology [113] and also for reliable industrial production. Apart from well-known advantages for protein expression, such as eukaryotic proteolytic processing, protein folding, disulfide bond formation and glycosylation, another factor contributing to Pichia pastoris outstanding popularity is its ability to secrete heterologous proteins while secreting very low levels of endogenous proteins. This allows extracellular accumulation of heterologously expressed soluble proteins, but also offers a route for production of eukaryotic membrane proteins as well, as they are efficiently trafficked through ER and Golgi to the plasma membrane.

Versatility of Pichia pastoris as host for membrane protein expression has been documented by the number of structures elucidated with Pichia-derived material (Table 1). In particular, a success rate of 93,5% has been found for expression of GPCRs, whereas more than half of all 100 proteins tested failed to be properly expressed in E. coli [26]. A closer analysis of specific binding activities also demonstrated that Pichia pastoris can keep up with higher eukaryotic systems, e.g. Semliki Forest virus-mediated expression in mammalian cells, but also showed that the ideal host is target dependent.

Thus, using complementary hosts allows to expand the expression space. If eukaryotic membrane proteins fail to be properly expressed in yeasts, attention is usually drawn to higher eukaryotic hosts, e.g. insect cells, mammalian cells or cell-free expression systems [114116]. These expression hosts are not covered by this review, but are outlined in detail in recent articles[26, 117, 118].

2. Strategies for membrane protein overexpression and problems encountered therein

Like for soluble proteins, each membrane protein behaves in an individual, unfortunately unpredictable way upon overexpression. In previous studies, no correlation between the "expressability" of a membrane protein and protein specific parameters, i.e. size, number of transmembrane helices, hydrophobicity, was found during homologous overexpression of 300 membrane proteins in E. coli ([119], reviewed in [120]). Other studies pointed out that heterologous expression of GPCRs in E. coli is limited to a size of 54 kDa and below [26]. Similarly, in S. cerevisiae, one of the most significant factors affecting the expression level was considered to be the molecular size of the protein - smaller proteins (< 60 kDa) generally tend to be better expressed than larger ones, as judged from homologous overexpression of more than 1000 membrane proteins in S. cerevisiae [84]. White and coworkers also found an inverse correlation between the number of transmembrane helices and the expression level, but presence of large extramembraneous domains might ameliorate a membrane protein's performance [84]. Highest expression levels were obtained for proteins with less than five transmembrane segments - preferentially composed of hydrophobic residues and lacking charged amino acids. Recently, in a "discovery-oriented" selection process, 234 out of 384 endogenous integral membrane proteins representing every IMP Pfam family within the yeast genome were successfully expressed under control of the GAL1 promoter in S. cerevisiae corresponding to a success rate of 61% with expression levels ranging from 0.5 to 5.8 mg L-1 [79]. Furthermore 25% of all candidate proteins were amenable to purification using n-Dodecyl-β-D-maltoside, as judged from immunoblotting of membrane extracts and the protein's performance during size-exclusion chromatography. Like in previous studies, the success rate for expression of integral membrane proteins was tightly linked to their specific properties. Best expression levels were obtained for small proteins (MW < 100 kDa) with a low number of transmembrane helices (<6) and a low average hydrophobicity index [79]. For heterologous proteins comparative studies are missing. However, a general trend was that proteins perform better during heterologous expression when related homologous proteins are present in the respective expression host [121]. However, most strategies towards optimization of membrane protein expression focused on modifying the protein itself and optimizing cultivation conditions rather than engineering the expression host.

2.1. Engineering membrane proteins for increased stability, affinity or activity

Improvements in expression levels can also be achieved by modifying the membrane protein. For the purpose of crystallization, the protein structure can be stabilized by increasing rigidity, e.g. through introduction of disulfide bonds [122] or N- and/or C-terminal truncations [11]. Furthermore, target proteins may be tailored by incorporation of point mutations with the aim to destroy biological activity and, thus, to diminish toxicity during heterologous overexpression [123]. In this regard, directed evolution strategies have turned out to be more straightforward compared to rational engineering, as the latter relies on structural information which is still scarce for membrane proteins. By employing directed evolution, expression levels, stability and binding selectivity of detergent-solubilized membrane proteins have been improved [124, 125]. Variants of the turkey β1-adrenergic receptor with improved conformational homogeneity in presence of antagonist, enhanced tolerance to short-chain detergents and thermostability have been obtained by alanine scanning followed by in-depth mutagenesis and combination of hot spots in E. coli [126].

To date, screening for improved variants or enhanced expression level has been almost exclusively carried out in E. coli, by employing immunodetection (colony-filtration blot of membranes) [127], FACS in the presence of specific fluorescent ligands [125] or specific activity [124] and ligand binding assays [126, 128]. Like for soluble proteins, activity-based screens allow to select for functional mutants [124], while screens relying on total expression levels including all immunodetection-based assays might preferentially enrich inactive, hence non-toxic proteins. Use of membranes instead of whole cells in combination with activity assays can circumvent the specified troubles, as suggested by Molina and coworkers [129]. Following initial screening using E. coli, selected variants are transferred to eukaryotic systems for production purposes [125]. Besides their impact on protein stability and function, mutations might directly affect transcriptional, translational and/or folding efficiency. In respect to differences in cellular milieus in between species, many promising candidates might fail in providing the same properties they have been selected for during the initial screening in prokaryotes. Recently, the suitability of S. cerevisiae to perform directed evolution experiments has been demonstrated, by improving ligand sensitivity of a human UDP-glucose receptor [130]. Meanwhile, the availability of protocols paves the way for the use of various yeast species as hosts in directed evolution experiments [85, 131].

2.2. Adaptation of the host to membrane protein production

2.2.1. Relieving metabolic stress evoked by membrane protein overexpression by adjusting transcription and translation efficiency to membrane protein folding

Apart from engineering proteins of interest, expression of membrane proteins can be fine-tuned on different cellular levels in order to improve yields. During production of membrane proteins high gene dosage strategies often fail in providing more functional protein but rather entail impaired growth or accumulation of aggregated protein in inclusion bodies as a result of limited cellular capacity to correctly translocate, assemble, modify and integrate proteins into the membrane [39, 132135]. As transcript abundance does not limit membrane protein production [136], assembly of membrane proteins often works better when synthesis rates are slowed down to better match the rates of insertion and assembly. Frequently, a high copy number entails an increase in total yield, but not in amounts of functional protein, as a consequence of improper balance of protein biosynthesis and folding [135, 137, 138]. Low transcriptional rates can be achieved by lowering the gene dosage or switching to weak, yet tightly regulated promoters, thereby avoiding accumulation of aggregated protein [38]. As a consequence of membrane protein production, cell growth is often retarded, thus inducible promoter systems may be superior to constitutive ones in membrane protein production (e.g. PBAD and PT7 for E. coli, PAOX1 for Pichia pastoris), as they allow unimpaired cell growth to high densities prior to protein expression. Apart from low gene dosage or weak promoters, expression kinetics can be fine-tuned by shortening induction periods, reducing inducer concentrations or switching to weak inducers, e.g. lactose for the T7 promoter [132, 139, 140].

If transcription efficiency limits the final yield, use of well-expressing genes in bicistronic expression constructs might be exploited to increase mRNA levels [141]. Efficiency of transcription initiation can be mediated by adapting the codon usage of the 5' region of the recombinant gene to the host's own one, but can also be improved by fusing well-expressed genes, encoding for e.g. β-galactosidase upstream of the gene of interest [142].

Another way to guide the protein along the secretory route to the plasma membrane is the use of N-terminal, host-specific secretory targeting sequences, e.g. of the Ste2 receptor [88, 143], the prepropeptide of the S. cerevisiae α-mating factor or the signal peptide of acid phosphatase [26, 135138, 144149]. The majority of integral membrane proteins (IMPs) however possesses a native N-terminal signal sequence, thus the use of N-terminal tags - either for detection by immunoblotting or for purification - might lead to delusive conclusions due to processing of the signal peptide [79]. When information on protein topology is scarce, the use of N-terminal secretory signal sequences might also interfere with protein folding and insertion into the membrane. This strategy, however, usually worked for GPCRs, where the N-terminus is facing the outward side of the membrane [150]. Apart from signal sequences, also N- or C-terminal fusions with soluble cytoplasmic (GFP, glutathione S-transferase) and periplasmic proteins (maltose binding protein) may improve expression of otherwise poorly expressed targets and promote their stabilization in E. coli, putatively by protecting membrane proteins against proteolytic degradation of vulnerable N- or C-termini [151155]. In this context, targeting to and integration into bacterial membranes has also been facilitated by fusion to other membrane proteins (maltoporin, glycerol-conducting channel GlpF, mistic) [142, 156]. Due to its ability to integrate into the membrane independently of the translocon, mistic, an integral 13 kDa membrane protein derived from Bacillus subtilis, can be used to eliminate bottlenecks encountered therein [157, 158]. Evidently, topologies of both membrane proteins - target protein and fusion partner - have to be considered, e.g. the N-terminal fusion of GlpF is limited to membrane proteins with N-termini facing the cytoplasm [156].

Finally, external parameters considerably affect transcription and translation rates, cultivation temperature being recognized as the most effective one. Generally, best growth conditions in terms of biomass yield are not necessarily ideal for heterologous protein expression, but might rather elicit a stress response [159] or result in low yield of functional membrane protein [144, 160]. In fact, folding and membrane insertion of the protein can be promoted by lowering the cultivation temperature [140, 144, 149, 160, 161]. At low temperature the activity of the transcriptional and translational apparatus is reduced, avoiding an overload thereof. Additionally, many cold-shock chaperones are induced at lower temperature, which promotes folding [162], but also reduces proteolytic degradation [163, 164]. The positive effect might further be linked to higher protein stability at low temperatures, but also to decreased folding stress. Especially in prokaryotes, folding of eukaryotic membrane proteins benefits from reduced transcription and translation rates as a result of adaptation to eukaryotic translation rates.

Effects of other external parameters, i.e. pH, osmolarity and aeration, on membrane protein expression have not been studied thoroughly so far. Only the influence of pH on the yield of individual membrane proteins has been documented for yeast, suggesting optimal values ranging from neutral to alkaline pH [160, 161]. These studies can not serve as general guidelines, however. Optimization is required for each target protein.

2.2.2. Relieving folding and translocation stress
The gross majority of membrane proteins follow the same route like soluble, secretory proteins once the nascent polypeptide emerges from the ribosome, including targeting to the translocon via the SRP particle (Figure 1, Figure 2). In contrast to secretory proteins, however, the most prominent bottleneck in overexpression of membrane proteins is the physical space within or at a lipid bilayer. Difficulties arise from limitations in membrane capacity when accommodating additional proteins. Each membrane has an optimal ratio between lipids and membrane proteins. Thus, variations caused by massive protein insertion affect membrane integrity and cell functionality [165]. Upon disturbance of this balance, expression systems often react with stress responses including protein degradation.
Figure 1

Membrane protein biogenesis in prokaryotes. In prokaryotes, most membrane proteins are targeted to and inserted into the cytoplasmic membrane by the SRP pathway, which involves interaction of the growing polypeptide chain with the signal recognition particle (SRP) and its receptor FtsY, binding of the nascent polypeptide chain-ribosome-complex to the SecYEG/YidC pore, translocation of cytoplasmic and periplasmic loops across the cytoplasmic membrane and their folding by SecA and various chaperones and insertion of hydrophobic segments into the membrane. The autonomous, YidC and Tat pathways, that are used by small proteins and membrane-associated periplasmic proteins, respectively, are mentioned here for sake of completeness.
Figure 2

Membrane protein biogenesis in eukaryotes. In eukaryotic cells, membrane protein biogenesis occurs in a cotranslational way. Proteins residing in membranes of ER and Golgi apparatus or in plasma membrane use the secretory pathway. Like in prokaryotes, SRP recognizes polypeptides protruding from the ribosome complex, thereby transiently attenuating translation. As soon as the SRP-ribosome complex interacts with the SRP receptor and docks to the Sec61 translocon pore, translation resumes, BiP relocates, thereby opening the lumenal gate and the membrane protein enters the membrane by lateral diffusion through the Sec61 pore. Peroxisomal membrane proteins either use the Pex19/Pex3-mediated way (class I proteins, shown here) or are thought to reach the peroxisomal membrane via the ER (class II) [208]. Mitochondrial membrane proteins pass through the outer mitochondrial membrane (OMM) via the TOM complex (translocase of the outer membrane). While β-barrel proteins of the OMM are transported to the SAM and MDM complexes (sorting and assembly machinery), the TIM22 and TIM23 complexes (translocase of the inner mitochondrial membrane) are used to target proteins to the inner mitochondrial membrane [209].


In prokaryotes, the SRP guides a nascent polypeptide chain to its membrane-associated receptor FtsY and subsequently to the Sec translocon consisting of the protein conducting channel SecY, SecE and SecG [166]. Sec translocon-mediated insertion into the cytoplasmic membrane is supported by the peripherally associated ATPase SecA, which is required for translocation of periplasmic loops and secretory proteins, and by YidC, which is thought to mediate lateral transport of transmembrane helices (TMH) into the membrane (Figure 1). Two proteases residing in the cytoplasmic membrane, FtsH and HtpX, play a crucial role in quality control of membrane proteins [167].

During membrane protein production, enhanced levels of folding proteins might be required in order to cope with the membrane protein load. As a shortage of foldases might limit the cellular productivity, membrane protein production can be optimized by providing surplus compounds of the assembly machinery. The effect of coexpression and deletion of chaperones and proteases has been recently investigated for E. coli expressing GPCRs [168, 169]. Using the human cannabinoid receptor CB1 as model protein, a transposon library of E. coli was screened for increased expression levels [169]. Inactivation of DnaJ (dnaJ::Tn5) resulted in a higher abundance of membrane-integrated receptor and also abolished growth-retarding effects of overexpression. On the other hand, coexpression of DnaJ/K during expression of the magnesium transporter CorA increased expression levels, and its role in membrane protein assembly has been ascribed to its capability to prevent accumulation of the protein in inclusion bodies [170]. From X-ray structural analysis, evidence emerged that presence of a large extramembraneous domain requires an increased amount of chaperones to mediate its folding [171]. The exact role of DnaJ during CB1 expression is not clear. According to topology predictions, the receptor lacks any large loops connecting its 7 TMHs. However, the N-terminal 116 amino acids were found to be located on the extracellular side, while the shorter C-terminal domain faces the cytoplasm. It has thus been speculated that the inhibitory role of DnaJ is linked to its ability to interact with the N-terminus proceeding from the ribosome, thus preventing its insertion into the Sec translocon [169]. Given that only total amounts of receptor are indicated, it remains to be clarified, whether non-functional and, thus, non-toxic protein has accumulated in the membrane due to absence of folding chaperones or whether the positive effect of dnaJ knockout is due to its strong interaction with the N-terminal region. Apart from dnaJ, positive effects on membrane protein biogenesis have also been observed upon inactivation of the transcription factor nhaR, which regulates expression of genes involved in cation transport and of the DNA damage-inducible helicase dinG. Yet, their precise role during membrane protein biogenesis need to be elucidated in detail [169]. Judging from the expression yields obtained for other membrane proteins (human CB2 receptor, human bradykinin receptor 2, human neurokinin receptor 1), the length of the N-terminal tail seems to play a crucial role, as no improvement has been achieved by transposon-mediated dnaJ inactivation.

Another study addressed the effect of coexpression of different chaperones, translocon compounds and proteases on membrane protein biogenesis, exemplified for the central and peripheral cannabinoid receptor (CB1 and CB2), the bradykinin receptor 2 (BR2) and the neurokinin-(substance 1) receptor 1 (NKR1) [168]. While many chaperones including the membrane integrase YidC, SRP compound 4.5S RNA, SRP receptor FtsY, compounds of the translocon SecY and SecE and the chaperones SecB, GroEL/GroES did not promote membrane protein production, a moderate increase in expression levels of CB1 has been achieved by coexpression of the SRP compound Ffh, chaperones DnaJ/K and the peptidyl-prolyl isomerase trigger factor Tig - thus opposing the previous study [169]. Unexpectedly, highest expression levels were obtained upon coexpression of FtsH, a membrane-anchored AAA+ protease [169]. Besides improved amounts of membrane-inserted receptor, a two-fold higher cell density provided evidence that cells experienced less stress, although cell division was impaired as shown by cell elongation. The fact that no improvement in binding efficiency of GPCRs was achieved and strains reached higher cell densities compared to control strains left a few questions unanswered. FtsH is involved in quality control of membrane proteins, however no effect has been observed for other AAA+ proteases (HtpX, YcaL, YfgC, and YggG). Preliminary results of a transcriptome analysis indicated that glycerol metabolism was largely rearranged in mutant strains, suggesting that the lipid composition of cytoplasmic membranes was altered [168]. Recent studies examined the stress response upon CB1 or FtsH production and revealed an induction of genes from the σ32 heat shock regulon [172]. Using promoter-GFP fusions, it was demonstrated that coexpression of CB1 and FtsH resulted in additive stress responses as assessed by flow cytometry, clearly indicating that FtsH is not able to attenuate stress responses caused by CB1 expression. Instead, stress-related effects were boosted further by FtsH coexpression. Authors proposed that this protease likely proactively prepares the cells to cope with the toxic effects caused by CB1.


Typically, membrane proteins - excluding proteins destined for peroxisomal, chloroplast and mitochondrial membranes - enter the secretory pathway by translocating into the ER membrane where folding and maturation of the proteins take place [68, 173, 174]. Like in prokaryotes, as soon as the signal sequence protrudes from the the growing polypeptide-ribosome complex, the SRP guides the complex to the ER membrane (Figure 2). Translation resumes when the complex docks to the Sec61p pore, triggering opening of the lumenal BiP-mediated gate. Yeast cells deploy several mechanisms to cope with the increased membrane protein load. Overproduction of ER-resident membrane proteins triggers enhanced proliferation of ER membranes as shown for HMG-CoA reductase and CYP52 A3, mediated by induction of the unfolded protein response [175177]. At the same time, ER chaperones act in concert to properly assemble membrane proteins or promote folding of lumenal, extramembraneous domains, thus their coexpression can boost ER folding capacity. Previously, expression levels of a serotonin transporter in the baculovirus expression system were improved by a factor of three upon coexpression of the ER-resident chaperone calnexin [178]. As this membrane protein requires the presence of a distinct N-glycan moiety to mature into functional protein, increased levels of calnexin were required to ensure efficient N-glycosylation within the ER. Coexpression of calreticulin and BiP also increased the final yield, albeit to a lesser extent. Similarly, increased abundance of the dnaK-type chaperone BiP mRNA has been found during overexpression of cytochrome P450 52A3 in S. cerevisiae [176, 177] and of the 2-compound cytochrome P450 system including P450 reductase and benzoate p-hydroxylase BphA in A. niger [179]. On the other hand, deletion of Cne1, a yeast homolog of mammalian calnexin and calreticulin, resulted in higher levels of human transferrin receptor in S. cerevisiae [180]. As part of the ER quality system, calnexin was thought to prevent transport of the human transferrin receptor to the plasma membrane, which was then reversed by CNE1 deletion. Furthermore, increased levels of Sec61 translocon have been observed during membrane protein production [177]. Folding of transmembrane segments is largely mediated by membrane-resident chaperones, which often display a high substrate specificity. Folding of amino acid permeases, hexose transporters, phosphate transporters and chitin synthase III was facilitated by chaperones Shr3, Gsf2, Pho86 and Chs7 respectively [181183]. Deletion of the respective chaperone resulted in protein aggregation and failure of proteins to exit the ER [182].

Besides mediating membrane protein folding, the ER serves as a quality checkpoint to control protein integrity before the protein exits the ER. If cellular capacities to correctly assemble membrane proteins are exhausted, aberrant protein accumulates within the ER and is subjected to different rescue or degradation routes. Eukaryotic cells employ different strategies to cope with the accumulation of misfolded proteins within the ER. First, inhibition of translation initiation counteracts further accumulation of unfolded polypeptides. Secondly, under conditions of increased membrane protein load, cells overcome folding limitations by upregulating expression of chaperones, thereby increasing the folding capacity within the ER [184]. The increased chaperone requirement in turn often triggers induction of the UPR, an intracellular signalling pathway that acts to relieve stress situations [185, 186]. Finally, proteins that fail to reach their native fold are targeted to the proteasome for degradation, through dislocation to the cytoplasm and protein ubiquitination. Depending on the topology and location of the misfolded domain, different pathways are employed for membrane protein turnover. While proteins with large cytosolic domains enter the Doa10-dependent route, lumenally exposed lesions target the protein to the Hrd1 degradation pathway [187191].

Being an indicator for folding problems and ER stress, the UPR has also been rationally exploited as a sensing mechanism allowing optimized production of functional membrane proteins in S. cerevisiae [186]. The trypanosomal H+/adenosine cotransporter was used as model protein and β-galactosidase as reporter with a transcriptional UPR element driving expression of the lacZ gene. Expression conditions were optimized for the transporter by minimizing UPR activation. This strategy, however, only works for membrane proteins that elicit the UPR upon overproduction as observed for evolutionarily divergent proteins, while most proteins from more closely related organisms, e.g. yeast receptor and plant transport proteins, did not highlight any folding problems.

2.2.3. Increasing protein stability by chemical chaperones

Membrane proteins often associate with specific compounds in vivo, be it defined lipids or interacting proteins, and their presence is crucial for proper folding, activity and/or stability. In this context, the subcellular localization plays a significant role. Many mitochondrial membrane proteins tightly interact with cardiolipin, as shown by their association in protein crystals even after the protein has been subjected to several purification steps [192, 193]. Thus, shortage or even lack of defined lipid molecules may affect heterologous expression of membrane proteins. Lipid compositions vary between different hosts and organelles (reviewed by [36]). For full activity, it is often crucial to keep the membrane protein in a similar environment as in its native host, e.g. by targeting it to the proper organelle or by choosing a related host. Membrane proteins may assemble into supercomplexes in vivo [194]. Thus, co-expression of proteins that are known to form stable complexes or tightly interact with the target protein might also improve overexpression. For example, the coexpression of human β2-adrenergic receptor and its corresponding mammalian G protein subunit in S. cerevisiae did not only improve stability, but was also necessary for in vivo functionality [143]. Similarly, small chemical ligands can reduce conformational flexibility by tight association, and thus decrease the likelihood of hydrophobic domains to be exposed and attacked by proteases or becoming prone to aggregation. This idea has been successfully applied in heterologous expression of GPCRs. By addition of specific ligands at concentrations close to 100 times the Kd value during the induction phase, expression levels and stability of GPCRs were increased [135, 144, 149].

Apart from specific ligands, chemical supplements, e.g. DMSO, glycerol and histidine, are known to affect membrane protein expression positively as evaluated extensively for GPCRs [135, 144, 195]. The stimulating effect of DMSO at low concentrations (2.5% (v/v)) seems to be linked to its ability to modify the physical properties of membranes and membrane capacity by upregulating transcription of genes involved in lipid biosynthesis [196]. DMSO also increases the permeability of membranes and, thus, improves the access of externally added ligands to membrane proteins [197]. Like for many chaperones, use of DMSO is not a universal key to success, as adverse effects including downregulated expression and proteolysis have also been observed for plasma membrane transporters in yeasts [198]. Chaperoning activities and stabilization of protein conformation, especially of glycoproteins, have been ascribed to glycerol. Addition of 10% (v/v) glycerol during growth led to an increase in expression levels, exemplified for a human P-glycoprotein during heterologous expression in S. cerevisiae [195]. Glycerol was thought to directly increase stability of the membrane protein. The positive influence of histidine, which is most often added at concentrations of 0.04 mg mL-1, is thought to be related to its ability to act as a physiological antioxidant, but the trivial possibility of improved availability of this amino acid can not be ruled out [199].

2.2.4. Rationalizing membrane protein production by engineering host cells

As membrane protein biogenesis requires a tight balance between different processes and even small changes might have far-reaching consequences the application of generally valid engineering approaches is complicated. In the past, attention had been chiefly drawn to modifications of cultivation conditions or of expression constructs, i.e. gene dosage, promoters, purification tags, leader sequences, fusion proteins, in order to optimize membrane protein production. If expression failed in an expression system a different expression host was investigated for its ability to correctly synthesize the protein. Experience has shown that many years of effort are necessary in order to succeed in protein crystallization. Many improvements have been achieved on a trial-and-error basis. Unfortunately, they did not provide any general guideline for membrane protein production, not to mention any insights into the physiological constraints host cells encounter. There are no great endeavours to adapt microbial expression hosts to membrane protein production. Instead, many labs have resorted to well-established protease-deficient strains in order to minimize proteolytic degradation rather than alleviating host-specific bottlenecks [77, 79, 144].

Low success rates and protein aggregation have sparked interest in the mechanisms and physiological effects of membrane protein biogenesis allowing identification of putative bottlenecks. Analysing the consequences of membrane protein production from a comprehensive molecular and cell biological view - accomplished on the transcriptome and/or proteome level - allows to study physiological effects, cellular constraints and stress regulation. Most importantly, the -omics approach will help to apply the compiled knowledge for rational engineering of the host strain. Although no general, single-key bottlenecks in membrane protein expression are known so far, factors like chaperones, foldases, proteases etc., which were found to facilitate membrane protein expression in single cases, are in focus of comprehensive molecular analyses of membrane protein overexpressing hosts by transcriptomics or proteomics. Several groups have already addressed the question whether genetic engineering of the host, going beyond simply shifting the rate-limiting step within one single metabolic pathway or process, can relieve specific bottlenecks. Classical engineering

The traditional way to improve heterologous hosts in terms of productivity is the classical strain engineering, involving chemical mutagens or UV radiation. In fact, so far only E. coli BL21(DE3) has been tailored for improved membrane protein production capacity by classical selection more than one decade ago [39]. After having recognized that overexpression of an oxoglutarate-malate carrier protein negatively affected cell growth, strains that were able to survive during protein expression were selected, termed Walker strains or C41(DE3) and C43(DE3). Interestingly, in these strains higher expression levels and unimpaired growth were observed upon overexpression of soluble and membrane proteins that otherwise hampered cell viability of BL21(DE3). Miroux and Walker also noted that lower transcript levels had been reached by the mutant strains compared to the BL21(DE3), suggesting that transcriptional rates had slowed down. Later, it was postulated that the high success rate of Walker strains was linked to their ability to proliferate additional intracellular membranes and, thus, tolerate increased membrane protein loads [54]. In order to decipher the mechanisms, which make these strains superior to conventional ones for membrane protein production, the proteome of the Walker strains overexpressing the prokaryotic membrane protein YidC was compared to the one obtained from the parental strain BL21(DE3) [38].

Although the Walker strains behaved superior regarding growth characteristics and final expression levels, the same proteome response was observed in all strains, thus giving no clue what was the key to success in the Walker strains. However, lower abundance of chaperones and proteases (ClpB, IbpA, HslUV) involved in resolving cytosolic aggregates indicated that in contrast to BL21(DE3) the Walker strains experienced fewer problems in folding and insertion of membrane proteins at the Sec translocon. Driven by many open questions, the de Gier group analyzed the genetic features of the strains in detail and discovered that the high success rate of the Walker strains in membrane protein expression likely originates from a lower transcriptional rate caused by reduced abundance of T7 RNA polymerase, which is used in these strains to drive recombinant protein expression. Mutations in the lacUV5 promoter, a strong variant of the wild-type lac promoter driving expression of the T7 RNA polymerase, have accumulated in these strains which decrease the promoter strength. As a result, transcription, translation and protein insertion into the membrane are well balanced. Cells more easily cope with the membrane protein load and accomodate them in a functional way into the cytoplasmic membrane [38]. The mutations leading to lower expression rate accumulated in the -10 region thereby reconverting the lacUV5 variant to the wildtype lac promoter, and in the lac operator region making the promoter susceptible to catabolite repression by glucose. The latter resulted in delayed expression. In turn, the de Gier lab has constructed engineered strains, designated Lemo21(DE3), which allow to control activity of T7 RNA polymerase by its inhibitor T7 lysozyme (T7Lys). In these strains, coexpression of T7Lys under control of the titrable rhamnose inducible promoter rhaBAD is exploited to rationally dampen T7 RNA polymerase activity. This strategy allows to fine-tune expression of soluble and membrane-embedded protein of both prokaryotic and eukaryotic origin in E. coli by avoiding conditions which result in aggregation of protein and recruitment of chaperones and proteases. Once again this study demonstrated that slowing down transcription is one key to success for membrane protein biogenesis. The use of -omics technologies to rationalize membrane protein production

Prokaryotic systems

Motivated by poor knowledge on the host's physiological response to membrane protein production, Wagner and coworkers systematically analysed the effect of overexpression of three different membrane proteins (YidC, YedZ, LepI) on the proteome of E. coli [200]. Overexpression of all model proteins hampered growth, resulting in early transition to stationary phase. According to flow cytometry, cells were slightly bigger, indicating increased proliferation of additional membranes to host foreign membrane proteins, but also impaired cell division. Other studies have also pointed out that E. coli cells overcome physical limitations by proliferating additional membranes in order to cope with the increased membrane protein load [201]. Judging from the proteome of cell lysate, protein aggregates and cytoplasmic membranes, it became clear that massive expression of membrane proteins severely disturbed protein homeostasis in the cytoplasm of E. coli [200]. In production strains, overloading of the translocon entailed an accumulation of cytoplasmic aggregates, thereby evoking sequestration of chaperones like DnaJ/K and GroEL/S as shown by immunoblotting. Increased abundance of proteolytic proteins (HslU/V, ClpXP, ClpB; assisting proteins IbpA/B) combined with higher levels of chaperones suggested that in response to membrane protein misfolding the heat shock reponse is activated. The recruitment of chaperones and proteases was required to reduce inclusion body formation and resolve overexpressed protein that had accumulated in inclusion bodies. As revealed by transcriptome analysis, transcription of heat shock genes (lon, ClpP, HslU/V) and molecular chaperones (DnaK, DnaJ) was upregulated in response to inclusion body formation [202, 203].

Besides the overexpressed membrane proteins, cytoplasmic aggregates contained chaperones, proteases (HslU/V, ClpXP), many essential cytoplasmic proteins and many precursors of periplasmic and outer membrane proteins, indicating that the capacity of the translocation machinery was saturated [200]. Therefore, coupling of transcription, translation and targeting needs to be properly balanced. In this specific case, protein aggregation was probably also evoked by the use of the strong promoter of the T7 polymerase which was employed to drive expression of the membrane proteins. The idea that membrane protein production exceeded the capacity of the Sec translocon was confirmed by different observations. On the one hand, secretion efficiency was reduced suggesting that cotranslational membrane protein biosynthesis competed with the posttranslational process of protein secretion. On the other hand, low levels of endogenous membrane proteins provided evidence that recombinant membrane protein outcompeted endogenous protein production, i.e. most prominently respiratory chain complexes. Increased levels of translocon components SecY, SecE and SecG and membrane-associated ribosomal subunit L5 however, inferred a saturation of the translocation capacity. Membrane protein overproduction compromised cellular respiration, as shown by reduced oxygen uptake rates and low cytochrome c oxidase activity. As a consequence of inefficient energy metabolism, the Arc two-component system was activated and the acetate-phosphotransacetylase pathway was primarily employed for ATP production. Interestingly, expression of all model proteins evoked similar responses on the proteome level, suggesting that E. coli faces similar bottlenecks during membrane protein expression irrespective of the protein. This sounds feasible as membrane proteins are typically overexpressed in the plasma membrane in prokaryotes, while in eukaryotic cells membrane proteins pass through and end up in different organelles and, thus, optimization approaches depend on the subcellular localization. It should be emphasized that depending on protein structure different, translocon-independent pathways might be used for targeting and membrane insertion in prokaryotes as observed for the magnesium transporter CorA [171]. This work also carries great promise for future host engineering and holds out the prospect that obstacles encountered in membrane protein production can be alleviated on a broad basis and do not require optimization for each individual protein. Based on the existing data, compounds of the translocon machinery are promising candidates for cell engineering with the aim to obtain higher productivity. Although not yet demonstrated, the authors also suggested the FtsH protease as putative target for knockout or inhibition. Alternatively, coexpressing FtsH inhibitors, e.g the peptide SpoVM derived from Bacillus subtilis, might improve membrane protein overexpression. However, this would conceptually contradict the unexpectedly positive effects of FtsH overexpression [169].

Yeast cells

The physiological response of yeast to membrane protein production has hardly been deciphered in a rational way. Some early studies aimed at considering membrane protein production in relation to cell physiology with the aim to minimize folding stress within the ER by circumventing induction of the UPR [186]. In order to reveal which factors govern membrane protein degradation and whether ER-localized membrane proteins follow the ERAD degradation route, a recent study analyzed the transcriptome of S. cerevisiae cells overexpressing a non-functional variant of the 12 TMH ABC transporter Ste6 [204]. Due to improper folding of the extramembraneous cytoplasmic domain and the transmembrane segments the protein accumulated within the ER membrane and was subjected to proteolytic degradation. The transcript profile provided evidence that the transcription factor Rpn4 played a prominent role in combating stress evoked by accumulation of misfolded membrane protein in the ER. Authors proposed a similar role for Rpn4 in degradation of ER-resident membrane proteins as attributed to UPR-transcription factor Hac1. During stress situations, the transcription factor Rpn4 regulates the expression of proteasomal genes and, thus, ensures survival of the cell.

Other studies have emphasized that conditions that are optimal for growth and high transcriptional rates rarely coincide with those for production of functional membrane proteins, which motivated Bonander and coworkers to study the differences between cultivation conditions in detail [160]. As target protein, the glycerol uptake/efflux facilitator protein Fps1p was homologously overexpressed in S. cerevisiae, and effects of temperature and pH on expression levels and mRNA availability were investigated. The study demonstrated that conditions favouring fast growth rate and high transcriptional activity do not promote membrane insertion of aquaglyceroporin Fps1 [160]. Improved levels of membrane-bound protein were achieved by shifting temperature to 20°C, thus slowing down growth rate. This was another piece of evidence that gene dosage and transcript abundance do not limit membrane protein expression. Motivated to decipher which mechanisms govern membrane protein biogenesis at different temperatures and pH, transcriptomes of expression strains cultivated at 30°C (pH 5) and 35°C (pH 5 and pH 7) were compared. Already a temperature shift of 5°C had a strong impact on the transcriptome, especially on transcript abundance of proteins involved in secretion and yeast cellular physiology. Recently, also data for the most productive 20°C-grown cells were published [224]. Downregulation of genes encoding for intracellular protein trafficking (SEC62, APM3 - mediating Golgi-to-vacuole transport and vacuolar trafficking, VTC3 - vacuolar trafficking) and proteins involved in ribosome biogenesis and assembly (RPP1A, CGR1, BMS1) indicated that the secretory pathway was compromised [205]. From higher abundance of SRP102 transcripts encoding β subunit of SRP authors concluded that the translocon was overloaded. In response to heterologous membrane protein synthesis, sterol biosynthesis was found to be upregulated as indicated by increased levels of ERG9, while transcription of the heat shock protein HSP82 was induced in response to growth at 35°C. Increased levels of HSP82, however, might have been also required for correct insertion of membrane proteins. Following initial transcriptome analysis, authors investigated by which means expression of Fps1p can be improved in S. cerevisiae [206]. Among differently regulated and related genes, 43 genes were selected as initial targets to assess membrane protein biogenesis in respective deletion or overexpression strains. Assuming that the Sec translocon capacity was limited effects of SEC63 coexpression and SRP102 deletion were investigated, but no improvements were obtained [200]. Strongest effects were observed when the Fps1p channel was produced in yeast lacking compounds of the transcriptional Spt-Ada-Gcn5-Acetyl (SAGA) transferase (SPT3, GCN5) and co-activator complex (SRB5), yielding up to 70-fold improved Fps1p levels. The 1.8 MDa-complex is involved in regulation of RNA polymerase II-mediated transcription and provides an alternative route in recruiting the transcription machinery to promoters independently of general transcription factors [207]. The high membrane protein yield was found to be closely linked to an increase in BMS1 levels compared to the wildtype strain. Being a nucleolar protein, BMS1 plays a role in ribosome biogenesis regulating biosynthesis of the 40S subunit. In turn, authors investigated effects of Bms1p abundance on Fps1p production by employing the doxycycline-dependent titratable Tet promoter to adjust BMS1. An improvement of up to 137-fold was achieved when 5 times more BMS1 was provided compared to the wildtype. Similar effects were observed for other membrane proteins (human A2a receptor) and soluble proteins (GFP).

Yields of functional membrane and soluble proteins were also increased by altering the ratio of 60S and 40S ribosomal subunits from 1:1 to 2:1 via BMS1 regulation, corresponding to a shift in 25S to 18S ratio from 2:1 to 3:1. As shown by polysome profiling, higher levels of free 60S subunit were present in overexpressers, while 40S and 80S levels remained constant emphasizing that Bms1p regulates biosynthesis of the 60S subunit. The improved strains exhibited a slower growth rate, but were metabolically more efficient compared to standard strains as revealed by microcalorimetry. Ribosome biogenesis is one of the major consumers of cellular energy. By tuning BMS1 transcript levels in a doxycyclin-dependent manner yields of both membrane and soluble proteins were optimized, indicating, that each protein requires individual adjustment of the doxycyclin concentration and thus BMS1 levels to achieve best expression levels [206].


The past has shown that membrane proteins are not only tricky to handle once they have been solubilized, but first of all they are difficult to obtain in large amounts - even by overexpression in heterologous hosts. Fortunately, published work provides insights into the mechanisms of membrane protein biogenesis so that many useful guidelines, hints and tips are available enabling us to improve the design of future experiments. Expression systems that are closely related to the target protein from a phylogenetic point of view provide a similar cellular milieu as the protein's native host. Accordingly, this holds also true for lipid compositions of membranes and protein processing machineries. Many recent advances in understanding membrane protein biogenesis and the role of specific lipids in correct folding and topology suggest that homologous overexpression is most promising to finally succeed in structure determination. An estimated 45% of all structures originate from homologous overexpression, thus homologous or closely related hosts have proven most feasible for membrane protein production [117]. Microbial systems, especially prokaryotic ones, in many cases might not fulfil the requirements for eukaryotic membrane proteins. However, membrane protein expression can be tuned by other means including gene design or slowing down transcriptional and translational rates by promoter and host engineering to match the ideal folding and assembly rates. One key strategy to remedy misfolding within the cell takes advantage of increased amounts of chaperones, thus guiding membrane proteins along its biogenesis and folding process.

The era of genomics has brought many exciting advances in membrane protein research. The available -omics technologies provide a complementary approach to decipher mechanisms underlying membrane protein biogenesis. By exploring the host-related molecular and physiological response, target proteins can be selected for rational host engineering. An exciting example is a recent report on the expression of eukaryotic membrane proteins in S. cerevisiae, allowing to obtain large amounts of both membrane-embedded and soluble proteins by tuning composition of ribosomal subunits [206]. Our basic understanding of membrane protein biogenesis is continuing to expand and thus offers exciting opportunities for future work. The breadth of recent progress in elucidation of membrane protein structure determination provides evidence that exciting years in membrane protein research lie ahead.

List of Abbreviations used


cytochrome P450


dimethyl sulfoxide


endoplasmic reticulum


Fluorescence Activated Cell Sorting


galactose kinase


UDP-glucose 4-epimerase


green fluorescent protein


G protein coupled receptor


high throughput


integral membrane protein


nuclear magnetic resonance


posttranslational modification


signal recognition particle


transmembrane helix


unfolded protein response.



The authors acknowledge the Fonds zur Wissenschaftlichen Forschung (FWF) for providing financial support for the PhD program "DK Molecular Enzymology" W901-B05.

Authors’ Affiliations

Institute of Molecular Biotechnology, Graz University of Technology
Austrian Centre for Industrial Biotechnology (ACIB), c/o Research Centre Applied Biocatalysis


  1. Warne T, Serrano-Vega MJ, Baker JG, Moukhametzianov R, Edwards PC, Henderson R, Leslie AG, Tate CG, Schertler GF: Structure of a beta1-adrenergic G-protein-coupled receptor. Nature. 2008, 454: 486-491. 10.1038/nature07101.
  2. Rasmussen SG, Choi HJ, Rosenbaum DM, Kobilka TS, Thian FS, Edwards PC, Burghammer M, Ratnala VR, Sanishvili R, Fischetti RF, Schertler GF, Weis WI, Kobilka BK: Crystal structure of the human beta2 adrenergic G-protein-coupled receptor. Nature. 2007, 450: 383-387. 10.1038/nature06325.
  3. Cherezov V, Rosenbaum DM, Hanson MA, Rasmussen SG, Thian FS, Kobilka TS, Choi HJ, Kuhn P, Weis WI, Kobilka BK, Stevens RC: High-resolution crystal structure of an engineered human beta2-adrenergic G protein-coupled receptor. Science. 2007, 318: 1258-1265. 10.1126/science.1150577.
  4. Hanson MA, Cherezov V, Griffith MT, Roth CB, Jaakola VP, Chien EY, Velasquez J, Kuhn P, Stevens RC: A specific cholesterol binding site is established by the 2.8 A structure of the human beta2-adrenergic receptor. Structure. 2008, 16: 897-905. 10.1016/j.str.2008.05.001.
  5. Jaakola VP, Griffith MT, Hanson MA, Cherezov V, Chien EY, Lane JR, Ijzerman AP, Stevens RC: The 2.6 angstrom crystal structure of a human A2A adenosine receptor bound to an antagonist. Science. 2008, 322: 1211-1217. 10.1126/science.1164772.
  6. Aller SG, Yu J, Ward A, Weng Y, Chittaboina S, Zhuo R, Harrell PM, Trinh YT, Zhang Q, Urbatsch IL, Chang G: Structure of P-glycoprotein reveals a molecular basis for poly-specific drug binding. Science. 2009, 323: 1718-1722. 10.1126/science.1168750.
  7. Nishida M, Cadene M, Chait BT, MacKinnon R: Crystal structure of a Kir3.1-prokaryotic Kir channel chimera. Embo J. 2007, 26: 4005-4015. 10.1038/sj.emboj.7601828.
  8. Jasti J, Furukawa H, Gonzales EB, Gouaux E: Structure of acid-sensing ion channel 1 at 1.9 A resolution and low pH. Nature. 2007, 449: 316-323. 10.1038/nature06163.
  9. Long SB, Campbell EB, Mackinnon R: Crystal structure of a mammalian voltage-dependent Shaker family K+ channel. Science. 2005, 309: 897-903. 10.1126/science.1116269.
  10. Long SB, Tao X, Campbell EB, MacKinnon R: Atomic structure of a voltage-dependent K+ channel in a lipid membrane-like environment. Nature. 2007, 450: 376-382. 10.1038/nature06265.
  11. Hiroaki Y, Tani K, Kamegawa A, Gyobu N, Nishikawa K, Suzuki H, Walz T, Sasaki S, Mitsuoka K, Kimura K, Mizoguchi A, Fujiyoshi Y: Implications of the aquaporin-4 structure on array formation and cell adhesion. J Mol Biol. 2006, 355: 628-639. 10.1016/j.jmb.2005.10.081.
  12. Tani K, Mitsuma T, Hiroaki Y, Kamegawa A, Nishikawa K, Tanimura Y, Fujiyoshi Y: Mechanism of aquaporin-4's fast and highly selective water conduction and proton exclusion. J Mol Biol. 2009, 389: 694-706. 10.1016/j.jmb.2009.04.049.
  13. Ho JD, Yeh R, Sandstrom A, Chorny I, Harries WE, Robbins RA, Miercke LJ, Stroud RM: Crystal structure of human aquaporin 4 at 1.8 A and its mechanism of conductance. Proc Natl Acad Sci USA. 2009, 106: 7437-7442. 10.1073/pnas.0902725106.
  14. Horsefield R, Norden K, Fellert M, Backmark A, Tornroth-Horsefield S, Terwisscha van Scheltinga AC, Kvassman J, Kjellbom P, Johanson U, Neutze R: High-resolution x-ray structure of human aquaporin 5. Proc Natl Acad Sci USA. 2008, 105: 13327-13332. 10.1073/pnas.0801466105.
  15. Tornroth-Horsefield S, Wang Y, Hedfalk K, Johanson U, Karlsson M, Tajkhorshid E, Neutze R, Kjellbom P: Structural mechanism of plant aquaporin gating. Nature. 2006, 439: 688-694. 10.1038/nature04316.
  16. Fischer G, Kosinska-Eriksson U, Aponte-Santamaria C, Palmgren M, Geijer C, Hedfalk K, Hohmann S, de Groot BL, Neutze R, Lindkvist-Petersson K: Crystal structure of a yeast aquaporin at 1.15 angstrom reveals a novel gating mechanism. PLoS Biol. 2009, 7: e1000130- 10.1371/journal.pbio.1000130.
  17. Williams PA, Cosme J, Vinkovic DM, Ward A, Angove HC, Day PJ, Vonrhein C, Tickle IJ, Jhoti H: Crystal structures of human cytochrome P450 3A4 bound to metyrapone and progesterone. Science. 2004, 305: 683-686. 10.1126/science.1099736.
  18. Williams PA, Cosme J, Ward A, Angove HC, Matak Vinkovic D, Jhoti H: Crystal structure of human cytochrome P450 2C9 with bound warfarin. Nature. 2003, 424: 464-468. 10.1038/nature01862.
  19. Rowland P, Blaney FE, Smyth MG, Jones JJ, Leydon VR, Oxbrow AK, Lewis CJ, Tennant MG, Modi S, Eggleston DS, Chenery RJ, Bridges AM: Crystal structure of human cytochrome P450 2D6. J Biol Chem. 2006, 281: 7614-7622. 10.1074/jbc.M511232200.
  20. Yano JK, Wester MR, Schoch GA, Griffin KJ, Stout CD, Johnson EF: The structure of human microsomal cytochrome P450 3A4 determined by X-ray crystallography to 2.05-A resolution. J Biol Chem. 2004, 279: 38091-38094. 10.1074/jbc.C400293200.
  21. White SH: The progress of membrane protein structure determination. Protein Sci. 2004, 13: 1948-1949. 10.1110/ps.04712004.
  22. Wallin E, von Heijne G: Genome-wide analysis of integral membrane proteins from eubacterial, archaean, and eukaryotic organisms. Protein Sci. 1998, 7: 1029-1038.
  23. Krogh A, Larsson B, von Heijne G, Sonnhammer EL: Predicting transmembrane protein topology with a hidden Markov model: application to complete genomes. J Mol Biol. 2001, 305: 567-580. 10.1006/jmbi.2000.4315.
  24. Negm RS, Pistole TG: The porin OmpC of Salmonella typhimurium mediates adherence to macrophages. Can J Microbiol. 1999, 45: 658-669. 10.1139/cjm-45-8-658.
  25. Soulas C, Baussant T, Aubry JP, Delneste Y, Barillat N, Caron G, Renno T, Bonnefoy JY, Jeannin P: Outer membrane protein A (OmpA) binds to and activates human macrophages. J Immunol. 2000, 165: 2335-2340.
  26. Lundstrom K, Wagner R, Reinhart C, Desmyter A, Cherouati N, Magnin T, Zeder-Lutz G, Courtot M, Prual C, Andre N, Hassaine G, Michel H, Cambillau C, Pattus F: Structural genomics on membrane proteins: comparison of more than 100 GPCRs in 3 expression systems. J Struct Funct Genomics. 2006, 7: 77-91. 10.1007/s10969-006-9011-2.
  27. Toyoshima C, Nakasako M, Nomura H, Ogawa H: Crystal structure of the calcium pump of sarcoplasmic reticulum at 2.6 A resolution. Nature. 2000, 405: 647-655. 10.1038/35015017.
  28. Stock D, Leslie AG, Walker JE: Molecular architecture of the rotary motor in ATP synthase. Science. 1999, 286: 1700-1705. 10.1126/science.286.5445.1700.
  29. Tsukihara T, Aoyama H, Yamashita E, Tomizaki T, Yamaguchi H, Shinzawa-Itoh K, Nakashima R, Yaono R, Yoshikawa S: The whole structure of the 13-subunit oxidized cytochrome c oxidase at 2.8 A. Science. 1996, 272: 1136-1144. 10.1126/science.272.5265.1136.
  30. Xia D, Yu CA, Kim H, Xia JZ, Kachurin AM, Zhang L, Yu L, Deisenhofer J: Crystal structure of the cytochrome bc1 complex from bovine heart mitochondria. Science. 1997, 277: 60-66. 10.1126/science.277.5322.60.
  31. Iwata S, Lee JW, Okada K, Lee JK, Iwata M, Rasmussen B, Link TA, Ramaswamy S, Jap BK: Complete structure of the 11-subunit bovine mitochondrial cytochrome bc1 complex. Science. 1998, 281: 64-71. 10.1126/science.281.5373.64.
  32. Gordon E, Horsefield R, Swarts HG, Pont JJ, Neutze R, Snijder A: Effective high-throughput overproduction of membrane proteins in Escherichia coli. Protein Expr Purif. 2008
  33. Tate CG, Haase J, Baker C, Boorsma M, Magnani F, Vallis Y, Williams DC: Comparison of seven different heterologous protein expression systems for the production of the serotonin transporter. Biochim Biophys Acta. 2003, 1610: 141-153. 10.1016/S0005-2736(02)00719-8.
  34. Granseth E, Seppala S, Rapp M, Daley DO, Von Heijne G: Membrane protein structural biology--how far can the bugs take us?. Mol Membr Biol. 2007, 24: 329-332. 10.1080/09687680701413882.
  35. Goder V, Junne T, Spiess M: Sec61p contributes to signal sequence orientation according to the positive-inside rule. Mol Biol Cell. 2004, 15: 1470-1478. 10.1091/mbc.E03-08-0599.
  36. Opekarova M, Tanner W: Specific lipid requirements of membrane proteins--a putative bottleneck in heterologous expression. Biochim Biophys Acta. 2003, 1610: 11-22. 10.1016/S0005-2736(02)00708-3.
  37. Widmann M, Christen P: Comparison of folding rates of homologous prokaryotic and eukaryotic proteins. J Biol Chem. 2000, 275: 18619-18622. 10.1074/jbc.C000156200.
  38. Wagner S, Klepsch MM, Schlegel S, Appel A, Draheim R, Tarry M, Hogbom M, van Wijk KJ, Slotboom DJ, Persson JO, de Gier JW: Tuning Escherichia coli for membrane protein overexpression. Proc Natl Acad Sci USA. 2008, 105: 14371-14376. 10.1073/pnas.0804090105.
  39. Miroux B, Walker JE: Over-production of proteins in Escherichia coli: mutant hosts that allow synthesis of some membrane proteins and globular proteins at high levels. J Mol Biol. 1996, 260: 289-298. 10.1006/jmbi.1996.0399.
  40. Engelhardt H, Meins T, Poynor M, Adams V, Nussberger S, Welte W, Zeth K: High-level expression, refolding and probing the natural fold of the human voltage-dependent anion channel isoforms I and II. J Membr Biol. 2007, 216: 93-105. 10.1007/s00232-007-9038-8.
  41. Bannwarth M, Schulz GE: The expression of outer membrane proteins for crystallization. Biochim Biophys Acta. 2003, 1610: 37-45. 10.1016/S0005-2736(02)00711-3.
  42. Quick M, Wright EM: Employing Escherichia coli to functionally express, purify, and characterize a human transporter. Proc Natl Acad Sci USA. 2002, 99: 8597-8601. 10.1073/pnas.132266599.
  43. Yamanaka K: Cold shock response in Escherichia coli. J Mol Microbiol Biotechnol. 1999, 1: 193-202.
  44. Blum A, Martin HJ, Maser E: Human 11beta-hydroxysteroid dehydrogenase 1/carbonyl reductase: recombinant expression in the yeast Pichia pastoris and Escherichia coli. Toxicology. 2000, 144: 113-120. 10.1016/S0300-483X(99)00197-3.
  45. Kaushal S, Ridge KD, Khorana HG: Structure and function in rhodopsin: the role of asparagine-linked glycosylation. Proc Natl Acad Sci USA. 1994, 91: 4024-4028. 10.1073/pnas.91.9.4024.
  46. Parcej DN, Eckhardt-Strelau L: Structural characterisation of neuronal voltage-sensitive K+ channels heterologously expressed in Pichia pastoris. J Mol Biol. 2003, 333: 103-116. 10.1016/j.jmb.2003.07.009.
  47. Gibson SK, Parkes JH, Liebman PA: Phosphorylation stabilizes the active conformation of rhodopsin. Biochemistry. 1998, 37: 11393-11398. 10.1021/bi980933w.
  48. Stanasila L, Lim WK, Neubig RR, Pattus F: Coupling efficacy and selectivity of the human mu-opioid receptor expressed as receptor-Galpha fusion proteins in Escherichia coli. J Neurochem. 2000, 75: 1190-1199. 10.1046/j.1471-4159.2000.0751190.x.
  49. Bertin B, Freissmuth M, Breyer RM, Schutz W, Strosberg AD, Marullo S: Functional expression of the human serotonin 5-HT1A receptor in Escherichia coli. Ligand binding properties and interaction with recombinant G protein alpha-subunits. J Biol Chem. 1992, 267: 8200-8206.
  50. Lee AG: How lipids affect the activities of integralmembrane proteins. Biochim Biophys Acta. 2004, 1666: 62-87. 10.1016/j.bbamem.2004.05.012.
  51. Hunte C: Specific protein-lipid interactions in membrane proteins. Biochem Soc Trans. 2005, 33: 938-942. 10.1042/BST20050938.
  52. Tate CG: Overexpression of mammalian integral membrane proteins for structural studies. FEBS Lett. 2001, 504: 94-98. 10.1016/S0014-5793(01)02711-9.
  53. Sharom FJ: The P-glycoprotein multidrug transporter: interactions with membrane lipids, and their modulation of activity. Biochem Soc Trans. 1997, 25: 1088-1096.
  54. Arechaga I, Miroux B, Karrasch S, Huijbregts R, de Kruijff B, Runswick MJ, Walker JE: Characterisation of new intracellular membranes in Escherichia coli accompanying large scale over-production of the b subunit of F(1)F(o) ATP synthase. FEBS Lett. 2000, 482: 215-219. 10.1016/S0014-5793(00)02054-8.
  55. Monne M, Chan KW, Slotboom DJ, Kunji ER: Functional expression of eukaryotic membrane proteins in Lactococcus lactis. Protein Sci. 2005, 14: 3048-3056. 10.1110/ps.051689905.
  56. Kunji ER, Chan KW, Slotboom DJ, Floyd S, O'Connor R, Monne M: Eukaryotic membrane protein overproduction in Lactococcus lactis. Curr Opin Biotechnol. 2005, 16: 546-551. 10.1016/j.copbio.2005.08.006.
  57. Kunji ER, Slotboom DJ, Poolman B: Lactococcus lactis as host for overproduction of functional membrane proteins. Biochim Biophys Acta. 2003, 1610: 97-108. 10.1016/S0005-2736(02)00712-5.
  58. Niu Y, Kong J, Xu Y: A novel GFP-fused eukaryotic membrane protein expression system in lactococcus lactis and its application to overexpression of an Elongase. Curr Microbiol. 2008, 57: 423-428. 10.1007/s00284-008-9223-8.
  59. Surade S, Klein M, Stolt-Bergner PC, Muenke C, Roy A, Michel H: Comparative analysis and "expression space" coverage of the production of prokaryotic membrane proteins for structural genomics. Protein Sci. 2006, 15: 2178-2189. 10.1110/ps.062312706.
  60. Quick M, Javitch JA: Monitoring the function of membrane transport proteins in detergent-solubilized form. Proc Natl Acad Sci USA. 2006, 104: 3603-3608. 10.1073/pnas.0609573104. 10.1073/pnas.0609573104.
  61. Turner GJ, Miercke LJ, Mitra AK, Stroud RM, Betlach MC, Winter-Vann A: Expression, purification, and structural characterization of the bacteriorhodopsin-aspartyl transcarbamylase fusion protein. Protein Expr Purif. 1999, 17: 324-338. 10.1006/prep.1999.1111.
  62. Turner GJ, Reusch R, Winter-Vann AM, Martinez L, Betlach MC: Heterologous gene expression in a membrane-protein-specific system. Protein Expr Purif. 1999, 17: 312-323. 10.1006/prep.1999.1110.
  63. Laible PD, Hata AN, Crawford AE, Hanson DK: Incorporation of selenomethionine into induced intracytoplasmic membrane proteins of Rhodobacter species. J Struct Funct Genomics. 2005, 6: 95-102. 10.1007/s10969-005-1936-3.
  64. Laible PD, Scott HN, Henry L, Hanson DK: Towards higher-throughput membrane protein production for structural genomics initiatives. J Struct Funct Genomics. 2004, 5: 167-172. 10.1023/B:JSFG.0000029201.33710.46.
  65. Drepper T, Arvani S, Rosenau F, Wilhelm S, Jaeger KE: High-level transcription of large gene regions: a novel T(7) RNA-polymerase-based system for expression of functional hydrogenases in the phototrophic bacterium Rhodobacter capsulatus. Biochem Soc Trans. 2005, 33: 56-58. 10.1042/BST0330056.
  66. Boer E, Steinborn G, Kunze G, Gellissen G: Yeast expression platforms. Appl Microbiol Biotechnol. 2007, 77: 513-523. 10.1007/s00253-007-1209-0.
  67. Martinez Molina D, Wetterholm A, Kohl A, McCarthy AA, Niegowski D, Ohlson E, Hammarberg T, Eshaghi S, Haeggstrom JZ, Nordlund P: Structural basis for synthesis of inflammatory mediators by human leukotriene C4 synthase. Nature. 2007, 448: 613-616. 10.1038/nature06009.
  68. Alder NN, Johnson AE: Cotranslational membrane protein biogenesis at the endoplasmic reticulum. J Biol Chem. 2004, 279: 22787-22790. 10.1074/jbc.R400002200.
  69. Boer H, Teeri TT, Koivula A: Characterization of Trichoderma reesei cellobiohydrolase Cel7A secreted from Pichia pastoris using two different promoters. Biotechnol Bioeng. 2000, 69: 486-494. 10.1002/1097-0290(20000905)69:5<486::AID-BIT3>3.0.CO;2-N.
  70. Choi BK, Jimenez-Flores R: Expression and purification of glycosylated bovine beta-casein (L70S/P71S) in Pichia pastoris. J Agric Food Chem. 2001, 49: 1761-1766. 10.1021/jf001298f.
  71. Hamilton SR, Bobrowicz P, Bobrowicz B, Davidson RC, Li H, Mitchell T, Nett JH, Rausch S, Stadheim TA, Wischnewski H, Wildt S, Gerngross TU: Production of complex human glycoproteins in yeast. Science. 2003, 301: 1244-1246. 10.1126/science.1088166.
  72. Hamilton SR, Davidson RC, Sethuraman N, Nett JH, Jiang Y, Rios S, Bobrowicz P, Stadheim TA, Li H, Choi BK, Hopkins D, Wischnewski H, Roser J, Mitchell T, Strawbridge RR, Hoopes J, Wildt S, Gerngross TU: Humanization of yeast to produce complex terminally sialylated glycoproteins. Science. 2006, 313: 1441-1443. 10.1126/science.1130256.
  73. Vervecken W, Callewaert N, Kaigorodov V, Geysens S, Contreras R: Modification of the N-Glycosylation Pathway to Produce Homogeneous, Human-Like Glycans Using GlycoSwitch Plasmids. Methods Mol Biol. 2007, 389: 119-138. full_text.
  74. Vervecken W, Kaigorodov V, Callewaert N, Geysens S, De Vusser K, Contreras R: In vivo synthesis of mammalian-like, hybrid-type N-glycans in Pichia pastoris. Appl Environ Microbiol. 2004, 70: 2639-2646. 10.1128/AEM.70.5.2639-2646.2004.
  75. Lagane B, Gaibelet G, Meilhoc E, Masson JM, Cezanne L, Lopez A: Role of sterols in modulating the human mu-opioid receptor function in Saccharomyces cerevisiae. J Biol Chem. 2000, 275: 33197-33200. 10.1074/jbc.C000576200.
  76. O'Malley MA, Lazarova T, Britton ZT, Robinson AS: High-level expression in Saccharomyces cerevisiae enables isolation and spectroscopic characterization of functional human adenosine A2a receptor. J Struct Biol. 2007, 159: 166-178. 10.1016/j.jsb.2007.05.001.
  77. Newstead S, Kim H, von Heijne G, Iwata S, Drew D: High-throughput fluorescent-based optimization of eukaryotic membrane protein overexpression and purification in Saccharomyces cerevisiae. Proc Natl Acad Sci USA. 2007, 104: 13936-13941. 10.1073/pnas.0704546104.
  78. Drew D, Newstead S, Sonoda Y, Kim H, von Heijne G, Iwata S: GFP-based optimization scheme for the overexpression and purification of eukaryotic membrane proteins in Saccharomyces cerevisiae. Nat Protoc. 2008, 3: 784-798. 10.1038/nprot.2008.44.
  79. Li M, Hays FA, Roe-Zurz Z, Vuong L, Kelly L, Ho CM, Robbins RM, Pieper U, O'Connell JD, Miercke LJ, Giacomini KM, Sali A, Stroud RM: Selecting optimum eukaryotic integral membrane proteins for structure determination by rapid expression and solubilization screening. J Mol Biol. 2009, 385: 820-830. 10.1016/j.jmb.2008.11.021.
  80. Ton VK, Rao R: Functional expression of heterologous proteins in yeast: insights into Ca2+ signaling and Ca2+-transporting ATPases. Am J Physiol Cell Physiol. 2004, 287: C580-589. 10.1152/ajpcell.00135.2004.
  81. Dreyer I, Horeau C, Lemaillet G, Zimmermann S, Bush DR, Rodriguez-Navarro A, Schachtman DP, Spalding EP, Sentenac H, Gaber RF: Identification and characterization of plant transporters using heterologous expression systems. J Exp Bot. 1999, 50: 1073-1087. 10.1093/jexbot/50.suppl_1.1073. 10.1093/jexbot/50.suppl_1.1073.
  82. Winzeler EA, Shoemaker DD, Astromoff A, Liang H, Anderson K, Andre B, Bangham R, Benito R, Boeke JD, Bussey H, Chu AM, Connelly C, Davis K, Dietrich F, Dow SW, El Bakkoury M, Foury F, Friend SH, Gentalen E, Giaever G, Hegemann JH, Jones T, Laub M, Liao H, Liebundguth N, Lockhart DJ, Lucau-Danila A, Lussier M, M'Rabet N, Menard P, Mittmann M, Pai C, Rebischung C, Revuelta JL, Riles L, Roberts CJ, Ross-MacDonald P, Scherens B, Snyder M, Sookhai-Mahadeo S, Storms RK, Veronneau S, Voet M, Volckaert G, Ward TR, Wysocki R, Yen GS, Yu K, Zimmermann K, Philippsen P, Johnston M, Davis RW: Functional characterization of the S. cerevisiae genome by gene deletion and parallel analysis. Science. 1999, 285: 901-906. 10.1126/science.285.5429.901.
  83. Osterberg M, Kim H, Warringer J, Melen K, Blomberg A, von Heijne G: Phenotypic effects of membrane protein overexpression in Saccharomyces cerevisiae. Proc Natl Acad Sci USA. 2006, 103: 11148-11153. 10.1073/pnas.0604078103.
  84. White MA, Clark KM, Grayhack EJ, Dumont ME: Characteristics affecting expression and solubilization of yeast membrane proteins. J Mol Biol. 2007, 365: 621-636. 10.1016/j.jmb.2006.10.004.
  85. Ito K, Sugawara T, Shiroishi M, Tokuda N, Kurokawa A, Misaka T, Makyio H, Yurugi-Kobayashi T, Shimamura T, Nomura N, Murata T, Abe K, Iwata S, Kobayashi T: Advanced method for high-throughput expression of mutated eukaryotic membrane proteins in Saccharomyces cerevisiae. Biochem Biophys Res Commun. 2008, 371: 841-845. 10.1016/j.bbrc.2008.04.182.
  86. Takegawa K, Tohda H, Sasaki M, Idiris A, Ohashi T, Mukaiyama H, Giga-Hama Y, Kumagai H: Production of heterologous proteins using the fission-yeast (Schizosaccharomyces pombe) expression system. Biotechnol Appl Biochem. 2009, 53: 227-235. 10.1042/BA20090048.
  87. Giga-Hama Y, Kumagai H: Expression system for foreign genes using the fission yeast Schizosaccharomyces pombe. Biotechnol Appl Biochem. 1999, 30 (Pt 3): 235-244.
  88. Arkinstall S, Edgerton M, Payton M, Maundrell K: Co-expression of the neurokinin NK2 receptor and G-protein components in the fission yeast Schizosaccharomyces pombe. FEBS Lett. 1995, 375: 183-187. 10.1016/0014-5793(95)01200-X.
  89. Sander P, Grunewald S, Reilander H, Michel H: Expression of the human D2S dopamine receptor in the yeasts Saccharomyces cerevisiae and Schizosaccharomyces pombe: a comparative study. FEBS Lett. 1994, 344: 41-46. 10.1016/0014-5793(94)00335-1.
  90. Bernhardt R: Cytochromes P450 as versatile biocatalysts. J Biotechnol. 2006, 124: 128-145. 10.1016/j.jbiotec.2006.01.026.
  91. Oeda K, Sakaki T, Ohkawa H: Expression of rat liver cytochrome P-450MC cDNA in Saccharomyces cerevisiae. DNA. 1985, 4: 203-210. 10.1089/dna.1985.4.203.
  92. Urban P, Werck-Reichhart D, Teutsch HG, Durst F, Regnier S, Kazmaier M, Pompon D: Characterization of recombinant plant cinnamate 4-hydroxylase produced in yeast. Kinetic and spectral properties of the major plant P450 of the phenylpropanoid pathway. Eur J Biochem. 1994, 222: 843-850. 10.1111/j.1432-1033.1994.tb18931.x.
  93. Sakaki T, Shibata M, Yabusaki Y, Murakami H, Ohkawa H: Expression of bovine cytochrome P450c21 and its fused enzymes with yeast NADPH-cytochrome P450 reductase in Saccharomyces cerevisiae. DNA Cell Biol. 1990, 9: 603-614. 10.1089/dna.1990.9.603.
  94. Truan G, Cullin C, Reisdorf P, Urban P, Pompon D: Enhanced in vivo monooxygenase activities of mammalian P450s in engineered yeast cells producing high levels of NADPH-P450 reductase and human cytochromeb5. Gene. 1993, 125: 49-55. 10.1016/0378-1119(93)90744-N.
  95. Zimmer T, Kaminski K, Scheller U, Vogel F, Schunck WH: In vivo reconstitution of highly active Candida maltosa cytochrome P450 monooxygenase systems in inducible membranes of Saccharomyces cerevisiae. DNA Cell Biol. 1995, 14: 619-628. 10.1089/dna.1995.14.619.
  96. Shibata M, Sakaki T, Yabusaki Y, Murakami H, Ohkawa H: Genetically engineered P450 monooxygenases: construction of bovine P450c17/yeast reductase fused enzymes. DNA Cell Biol. 1990, 9: 27-36. 10.1089/dna.1990.9.27.
  97. Dumas B, Cauet G, Lacour T, Degryse E, Laruelle L, Ledoux C, Spagnoli R, Achstetter T: 11 beta-hydroxylase activity in recombinant yeast mitochondria. In vivo conversion of 11-deoxycortisol to hydrocortisone. Eur J Biochem. 1996, 238: 495-504. 10.1111/j.1432-1033.1996.0495z.x.
  98. Ewen KM, Schiffler B, Uhlmann-Schiffler H, Bernhardt R, Hannemann F: The endogenous adrenodoxin reductase-like flavoprotein arh1 supports heterologous cytochrome P450-dependent substrate conversions in Schizosaccharomyces pombe. FEMS Yeast Res. 2008, 8: 432-441. 10.1111/j.1567-1364.2008.00360.x.
  99. Bureik M, Schiffler B, Hiraoka Y, Vogel F, Bernhardt R: Functional Expression of Human Mitochondrial CYP11B2 in Fission Yeast and Identification of a New Internal Electron Transfer Protein, etp1. Biochemistry. 2002, 41: 2311-2321. 10.1021/bi0157870.
  100. Dragan CA, Zearo S, Hannemann F, Bernhardt R, Bureik M: Efficient conversion of 11-deoxycortisol to cortisol (hydrocortisone) by recombinant fission yeast Schizosaccharomyces pombe. FEMS Yeast Res. 2005, 5: 621-625. 10.1016/j.femsyr.2004.12.001.
  101. Peters FT, Dragan CA, Wilde DR, Meyer MR, Zapp J, Bureik M, Maurer HH: Biotechnological synthesis of drug metabolites using human cytochrome P450 2D6 heterologously expressed in fission yeast exemplified for the designer drug metabolite 4'-hydroxymethyl-alpha-pyrrolidinobutyrophenone. Biochem Pharmacol. 2007, 74: 511-520. 10.1016/j.bcp.2007.05.010.
  102. Peters FT, Dragan CA, Schwaninger AE, Sauer C, Zapp J, Bureik M, Maurer HH: Use of fission yeast heterologously expressing human cytochrome P450 2B6 in biotechnological synthesis of the designer drug metabolite N-(1-phenylcyclohexyl)-2-hydroxyethanamine. Forensic Sci Int. 2009, 184: 69-73. 10.1016/j.forsciint.2008.12.001.
  103. Hakki T, Zearo S, Dragan CA, Bureik M, Bernhardt R: Coexpression of redox partners increases the hydrocortisone (cortisol) production efficiency in CYP11B1 expressing fission yeast Schizosaccharomyces pombe. J Biotechnol. 2008, 133: 351-359. 10.1016/j.jbiotec.2007.06.022.
  104. Juretzek T, Mauersberger S, Schnuck W-H, Nicaud J, Barth G: Functional expression of heterologous cytochrome P450 in the yeast Yarrowia lipolytica and its use in biotransformation of steroids. Curr Genet. 1999, 35: 307-
  105. Nthangeni MB, Urban P, Pompon D, Smit MS, Nicaud JM: The use of Yarrowia lipolytica for the expression of human cytochrome P450 CYP1A1. Yeast. 2004, 21: 583-592. 10.1002/yea.1127.
  106. Shiningavamwe A, Obiero G, Albertyn J, Nicaud JM, Smit M: Heterologous expression of the benzoate para-hydroxylase encoding gene (CYP53B1) from Rhodotorula minuta by Yarrowia lipolytica. Appl Microbiol Biotechnol. 2006, 72: 323-329. 10.1007/s00253-005-0264-7.
  107. Cereghino JL, Cregg JM: Heterologous protein expression in the methylotrophic yeast Pichia pastoris. FEMS Microbiol Rev. 2000, 24: 45-66. 10.1111/j.1574-6976.2000.tb00532.x.
  108. Cregg JM, Cereghino JL, Shi J, Higgins DR: Recombinant protein expression in Pichia pastoris. Mol Biotechnol. 2000, 16: 23-52. 10.1385/MB:16:1:23.
  109. Stewart MQ, Esposito RD, Gowani J, Goodman JM: Alcohol oxidase and dihydroxyacetone synthase, the abundant peroxisomal proteins of methylotrophic yeasts, assemble in different cellular compartments. J Cell Sci. 2001, 114: 2863-2868.
  110. Sreekrishna K, Brankamp RG, Kropp KE, Blankenship DT, Tsay JT, Smith PL, Wierschke JD, Subramaniam A, Birkenberger LA: Strategies for optimal synthesis and secretion of heterologous proteins in the methylotrophic yeast Pichia pastoris. Gene. 1997, 190: 55-62. 10.1016/S0378-1119(96)00672-5.
  111. Hollenberg CP, Gellissen G: Production of recombinant proteins by methylotrophic yeasts. Curr Opin Biotechnol. 1997, 8: 554-560. 10.1016/S0958-1669(97)80028-6.
  112. Nyblom M, Oberg F, Lindkvist-Petersson K, Hallgren K, Findlay H, Wikstrom J, Karlsson A, Hansson O, Booth PJ, Bill RM, Neutze R, Hedfalk K: Exceptional overproduction of a functional human membrane protein. Protein Expr Purif. 2007, 56: 110-120. 10.1016/j.pep.2007.07.007.
  113. Wood MJ, Komives EA: Production of large quantities of isotopically labeled protein in Pichia pastoris by fermentation. J Biomol NMR. 1999, 13: 149-159. 10.1023/A:1008398313350.
  114. Massotte D: G protein-coupled receptor overexpression with the baculovirus-insect cell system: a tool for structural and functional studies. Biochim Biophys Acta. 2003, 1610: 77-89. 10.1016/S0005-2736(02)00720-4.
  115. Higgins MK, Demir M, Tate CG: Calnexin co-expression and the use of weaker promoters increase the expression of correctly assembled Shaker potassium channel in insect cells. Biochim Biophys Acta. 2003, 1610: 124-132. 10.1016/S0005-2736(02)00715-0.
  116. Schwarz D, Klammt C, Koglin A, Lohr F, Schneider B, Dotsch V, Bernhard F: Preparative scale cell-free expression systems: new tools for the large scale preparation of integral membrane proteins for functional and structural studies. Methods. 2007, 41: 355-369. 10.1016/j.ymeth.2006.07.001.
  117. Junge F, Schneider B, Reckel S, Schwarz D, Dotsch V, Bernhard F: Large-scale production of functional membrane proteins. Cell Mol Life Sci. 2008, 65: 1729-1755. 10.1007/s00018-008-8067-5.
  118. Midgett CR, Madden DR: Breaking the bottleneck: eukaryotic membrane protein expression for high-resolution structural studies. J Struct Biol. 2007, 160: 265-274. 10.1016/j.jsb.2007.07.001.
  119. Daley DO, Rapp M, Granseth E, Melen K, Drew D, von Heijne G: Global topology analysis of the Escherichia coli inner membrane proteome. Science. 2005, 308: 1321-1323. 10.1126/science.1109730.
  120. Wang DN, Safferling M, Lemieux MJ, Griffith H, Chen Y, Li XD: Practical aspects of overexpressing bacterial secondary membrane transporters for structural studies. Biochim Biophys Acta. 2003, 1610: 23-36. 10.1016/S0005-2736(02)00709-5.
  121. Sarramegna V, Talmont F, Demange P, Milon A: Heterologous expression of G-protein-coupled receptors: comparison of expression systems fron the standpoint of large-scale production and purification. Cell Mol Life Sci. 2003, 60: 1529-1546. 10.1007/s00018-003-3168-7.
  122. Standfuss J, Xie G, Edwards PC, Burghammer M, Oprian DD, Schertler GF: Crystal structure of a thermally stable rhodopsin mutant. J Mol Biol. 2007, 372: 1179-1188. 10.1016/j.jmb.2007.03.007.
  123. Nitta T, Chiba A, Yamamoto N, Yamaoka S: Lack of cytotoxic property in a variant of Epstein-Barr virus latent membrane protein-1 isolated from nasopharyngeal carcinoma. Cell Signal. 2004, 16: 1071-1081.
  124. Zhou Y, Bowie JU: Building a thermostable membrane protein. J Biol Chem. 2000, 275: 6975-6979. 10.1074/jbc.275.10.6975.
  125. Sarkar CA, Dodevski I, Kenig M, Dudli S, Mohr A, Hermans E, Pluckthun A: Directed evolution of a G protein-coupled receptor for expression, stability, and binding selectivity. Proc Natl Acad Sci USA. 2008, 105: 14808-14813. 10.1073/pnas.0803103105.
  126. Serrano-Vega MJ, Magnani F, Shibata Y, Tate CG: Conformational thermostabilization of the beta1-adrenergic receptor in a detergent-resistant form. Proc Natl Acad Sci USA. 2008, 105: 877-882. 10.1073/pnas.0711253105.
  127. Molina DM, Cornvik T, Eshaghi S, Haeggstrom JZ, Nordlund P, Sabet MI: Engineering membrane protein overproduction in Escherichia coli. Protein Sci. 2008, 17 (4): 673-680. 10.1110/ps.073242508.
  128. Magnani F, Shibata Y, Serrano-Vega MJ, Tate CG: Co-evolving stability and conformational homogeneity of the human adenosine A2a receptor. Proc Natl Acad Sci USA. 2008, 105: 10744-10749. 10.1073/pnas.0804396105.
  129. Molina DM: Engineering membrane protein overproduction in Escherichia coli. Protein Sci. 2008
  130. Ault AD, Broach JR: Creation of GPCR-based chemical sensors by directed evolution in yeast. Protein Eng Des Sel. 2006, 19: 1-8. 10.1093/protein/gzi069.
  131. Liu Z, Pscheidt B, Avi M, Gaisberger R, Hartner FS, Schuster C, Skranc W, Gruber K, Glieder A: Laboratory evolved biocatalysts for stereoselective syntheses of substituted benzaldehyde cyanohydrins. Chembiochem. 2008, 9: 58-61. 10.1002/cbic.200700514.
  132. Geertsma ER, Groeneveld M, Slotboom DJ, Poolman B: Quality control of overexpressed membrane proteins. Proc Natl Acad Sci USA. 2008, 105: 5722-5727. 10.1073/pnas.0802190105.
  133. Lewinson O, Lee AT, Rees DC: The funnel approach to the precrystallization production of membrane proteins. J Mol Biol. 2008, 377: 62-73. 10.1016/j.jmb.2007.12.059.
  134. Grisshammer R, Tate CG: Overexpression of integral membrane proteins for structural studies. Q Rev Biophys. 1995, 28: 315-422. 10.1017/S0033583500003504.
  135. Weiss HM, Haase W, Reilander H: Expression of an integral membrane protein, the 5HT5A receptor. Methods Mol Biol. 1998, 103: 227-239.
  136. Sarramegna V, Talmont F, Seree de Roch M, Milon A, Demange P: Green fluorescent protein as a reporter of human mu-opioid receptor overexpression and localization in the methylotrophic yeast Pichia pastoris. J Biotechnol. 2002, 99: 23-39. 10.1016/S0168-1656(02)00161-X.
  137. Shukla AK, Haase W, Reinhart C, Michel H: Heterologous expression and characterization of the recombinant bradykinin B2 receptor using the methylotrophic yeast Pichia pastoris. Protein Expr Purif. 2007, 55: 1-8. 10.1016/j.pep.2007.02.021.
  138. Weiss HM, Haase W, Michel H, Reilander H: Expression of functional mouse 5-HT5A serotonin receptor in the methylotrophic yeast Pichia pastoris: pharmacological characterization and localization. FEBS Lett. 1995, 377: 451-456. 10.1016/0014-5793(95)01389-X.
  139. Gordon E, Horsefield R, Swarts HG, de Pont JJ, Neutze R, Snijder A: Effective high-throughput overproduction of membrane proteins in Escherichia coli. Protein Expr Purif. 2008, 62 (1): 1-8. 10.1016/j.pep.2008.07.005.
  140. Eshaghi S, Hedren M, Nasser MI, Hammarberg T, Thornell A, Nordlund P: An efficient strategy for high-throughput expression screening of recombinant integral membrane proteins. Protein Sci. 2005, 14: 676-683. 10.1110/ps.041127005.
  141. Mokhonova EI, Mokhonov VV, Akama H, Nakae T: Forceful large-scale expression of "problematic" membrane proteins. Biochem Biophys Res Commun. 2005, 327: 650-655. 10.1016/j.bbrc.2004.12.059.
  142. Marullo S, Delavier-Klutchko C, Eshdat Y, Strosberg AD, Emorine L: Human beta 2-adrenergic receptors expressed in Escherichia coli membranes retain their pharmacological properties. Proc Natl Acad Sci USA. 1988, 85: 7551-7555. 10.1073/pnas.85.20.7551.
  143. King K, Dohlman HG, Thorner J, Caron MG, Lefkowitz RJ: Control of yeast mating signal transduction by a mammalian beta 2-adrenergic receptor and Gs alpha subunit. Science. 1990, 250: 121-123. 10.1126/science.2171146.
  144. Andre N, Cherouati N, Prual C, Steffan T, Zeder-Lutz G, Magnin T, Pattus F, Michel H, Wagner R, Reinhart C: Enhancing functional production of G protein-coupled receptors in Pichia pastoris to levels required for structural studies via a single expression screen. Protein Sci. 2006, 15: 1115-1126. 10.1110/ps.062098206.
  145. Singh S, Gras A, Fiez-Vandal C, Ruprecht J, Rana R, Martinez M, Strange PG, Wagner R, Byrne B: Large-scale functional expression of WT and truncated human adenosine A2A receptor in Pichia pastoris bioreactor cultures. Microb Cell Fact. 2008, 7: 28- 10.1186/1475-2859-7-28.
  146. Zeder-Lutz G, Cherouati N, Reinhart C, Pattus F, Wagner R: Dot-blot immunodetection as a versatile and high-throughput assay to evaluate recombinant GPCRs produced in the yeast Pichia pastoris. Protein Expr Purif. 2006, 50: 118-127. 10.1016/j.pep.2006.05.017.
  147. Sarramegna V, Muller I, Mousseau G, Froment C, Monsarrat B, Milon A, Talmont F: Solubilization, purification, and mass spectrometry analysis of the human mu-opioid receptor expressed in Pichia pastoris. Protein Expr Purif. 2005, 43: 85-93. 10.1016/j.pep.2005.05.007.
  148. Yang G, Liu T, Peng W, Sun X, Zhang H, Wu C, Shen D: Expression and localization of recombinant human EDG-1 receptors in Pichia pastoris. Biotechnol Lett. 2006, 28: 1581-1586. 10.1007/s10529-006-9125-4.
  149. Fraser NJ: Expression and functional purification of a glycosylation deficient version of the human adenosine 2a receptor for structuralstudies. Protein Expr Purif. 2006, 49: 129-137. 10.1016/j.pep.2006.03.006.
  150. Wallin E, von Heijne G: Properties of N-terminal tails in G-protein coupled receptors: a statistical study. Protein Eng. 1995, 8: 693-698. 10.1093/protein/8.7.693.
  151. Halbhuber Z, Petrmichlova Z, Alexciev K, Thulin E, Stys D: Overexpression and purification of recombinant membrane PsbH protein in Escherichia coli. Protein Expr Purif. 2003, 32: 18-27. 10.1016/S1046-5928(03)00188-8.
  152. Grisshammer R, Duckworth R, Henderson R: Expression of a rat neurotensin receptor in Escherichia coli. Biochem J. 1993, 295 (Pt 2): 571-576.
  153. Hampe W, Voss RH, Haase W, Boege F, Michel H, Reilander H: Engineering of a proteolytically stable human beta 2-adrenergic receptor/maltose-binding protein fusion and production of the chimeric protein in Escherichia coli and baculovirus-infected insect cells. J Biotechnol. 2000, 77: 219-234. 10.1016/S0168-1656(99)00216-3.
  154. Drew D, Slotboom DJ, Friso G, Reda T, Genevaux P, Rapp M, Meindl-Beinker NM, Lambert W, Lerch M, Daley DO, Van Wijk KJ, Hirst J, Kunji E, De Gier JW: A scalable, GFP-based pipeline for membrane protein overexpression screening and purification. Protein Sci. 2005, 14: 2011-2017. 10.1110/ps.051466205.
  155. Berthold DA, Voevodskaya N, Stenmark P, Graslund A, Nordlund P: EPR studies of the mitochondrial alternative oxidase. Evidence for a diiron carboxylate center. J Biol Chem. 2002, 277: 43608-43614. 10.1074/jbc.M206724200.
  156. Neophytou I, Harvey R, Lawrence J, Marsh P, Panaretou B, Barlow D: Eukaryotic integral membrane protein expression utilizing the Escherichia coli glycerol-conducting channel protein (GlpF). Appl Microbiol Biotechnol. 2007, 77: 375-381. 10.1007/s00253-007-1174-7.
  157. Kefala G, Kwiatkowski W, Esquivies L, Maslennikov I, Choe S: Application of Mistic to improving the expression and membrane integration of histidine kinase receptors from Escherichia coli. J Struct Funct Genomics. 2007, 8: 167-172. 10.1007/s10969-007-9033-4.
  158. Roosild TP, Greenwald J, Vega M, Castronovo S, Riek R, Choe S: NMR structure of Mistic, a membrane-integrating protein for membrane protein expression. Science. 2005, 307: 1317-1321. 10.1126/science.1106392.
  159. Gasch AP, Werner-Washburne M: The genomics of yeast responses to environmental stress and starvation. Funct Integr Genomics. 2002, 2: 181-192. 10.1007/s10142-002-0058-2.
  160. Bonander N, Hedfalk K, Larsson C, Mostad P, Chang C, Gustafsson L, Bill RM: Design of improved membrane protein production experiments: quantitation of the host response. Protein Sci. 2005, 14: 1729-1740. 10.1110/ps.051435705.
  161. Sarramegna V, Demange P, Milon A, Talmont F: Optimizing functional versus total expression of the human mu-opioid receptor in Pichiapastoris. Protein Expr Purif. 2002, 24: 212-220. 10.1006/prep.2001.1564.
  162. Ferrer M, Chernikova TN, Yakimov MM, Golyshin PN, Timmis KN: Chaperonins govern growth of Escherichia coli at low temperatures. Nat Biotechnol. 2003, 21: 1266-1267. 10.1038/nbt1103-1266.
  163. Jahic M, Wallberg F, Bollok M, Garcia P, Enfors SO: Temperature limited fed-batch technique for control of proteolysis in Pichia pastoris bioreactor cultures. Microb Cell Fact. 2003, 2: 6- 10.1186/1475-2859-2-6.
  164. Phadtare S, Inouye M: Genome-wide transcriptional analysis of the cold shock response in wild-type and cold-sensitive, quadruple-csp-deletion strains of Escherichia coli. J Bacteriol. 2004, 186: 7007-7014. 10.1128/JB.186.20.7007-7014.2004.
  165. Drew D, Froderberg L, Baars L, de Gier JW: Assembly and overexpression of membrane proteins in Escherichia coli. Biochim Biophys Acta. 2003, 1610: 3-10. 10.1016/S0005-2736(02)00707-1.
  166. Luirink J, Sinning I: SRP-mediated protein targeting: structure and function revisited. Biochim Biophys Acta. 2004, 1694: 17-35.
  167. Akiyama Y: Quality control of cytoplasmic membrane proteins in Escherichia coli. J Biochem. 2009, 146 (4): 449-454. 10.1093/jb/mvp071.
  168. Link AJ, Skretas G, Strauch EM, Chari NS, Georgiou G: Efficient production of membrane-integrated and detergent-soluble G protein-coupled receptors in Escherichia coli. Protein Sci. 2008, 17: 1857-1863. 10.1110/ps.035980.108.
  169. Skretas G, Georgiou G: Genetic analysis of G protein-coupled receptor expression in Escherichia coli: inhibitory role of DnaJ on the membrane integration of the human central cannabinoid receptor. Biotechnol Bioeng. 2009, 102: 357-367. 10.1002/bit.22097.
  170. Chen Y, Song J, Sui SF, Wang DN: DnaK and DnaJ facilitated the folding process and reduced inclusion body formation of magnesium transporter CorA overexpressed in Escherichia coli. Protein Expr Purif. 2003, 32: 221-231. 10.1016/S1046-5928(03)00233-X.
  171. Eshaghi S, Niegowski D, Kohl A, Martinez Molina D, Lesley SA, Nordlund P: Crystal structure of a divalent metal ion transporter CorA at 2.9 angstrom resolution. Science. 2006, 313: 354-357. 10.1126/science.1127121.
  172. Xu LY, Link AJ: Stress responses to heterologous membrane protein expression in Escherichia coli. Biotechnol Lett. 2009, 31: 1775-1782. 10.1007/s10529-009-0075-5.
  173. Heinrich SU, Mothes W, Brunner J, Rapoport TA: The Sec61p complex mediates the integration of a membrane protein by allowing lipid partitioning of the transmembrane domain. Cell. 2000, 102: 233-244. 10.1016/S0092-8674(00)00028-3.
  174. Rapoport TA, Goder V, Heinrich SU, Matlack KE: Membrane-protein integration and the role of the translocation channel. Trends Cell Biol. 2004, 14: 568-575. 10.1016/j.tcb.2004.09.002.
  175. Wright R, Basson M, D'Ari L, Rine J: Increased amounts of HMG-CoA reductase induce "karmellae": a proliferation of stacked membrane pairs surrounding the yeast nucleus. J Cell Biol. 1988, 107: 101-114. 10.1083/jcb.107.1.101.
  176. Menzel R, Vogel F, Kargel E, Schunck WH: Inducible membranes in yeast: relation to the unfolded-protein-response pathway. Yeast. 1997, 13: 1211-1229. 10.1002/(SICI)1097-0061(199710)13:13<1211::AID-YEA168>3.0.CO;2-8.
  177. Wiedmann B, Silver P, Schunck WH, Wiedmann M: Overexpression of the ER-membrane protein P-450 CYP52A3 mimics sec mutant characteristics in Saccharomyces cerevisiae. Biochim Biophys Acta. 1993, 1153: 267-276. 10.1016/0005-2736(93)90415-V.
  178. Tate CG, Whiteley E, Betenbaugh MJ: Molecular chaperones stimulate the functional expression of the cocaine-sensitive serotonin transporter. J Biol Chem. 1999, 274: 17551-17558. 10.1074/jbc.274.25.17551.
  179. Dave A, Jeenes DJ, Mackenzie DA, Archer DB: HacA-independent induction of chaperone-encoding gene bipA in Aspergillus niger strains overproducing membrane proteins. Appl Environ Microbiol. 2006, 72: 953-955. 10.1128/AEM.72.1.953-955.2006.
  180. Prinz B, Stahl U, Lang C: Intracellular transport of a heterologous membrane protein, the human transferrin receptor, in Saccharomyces cerevisiae. Int Microbiol. 2003, 6: 49-55.
  181. Kota J, Gilstring CF, Ljungdahl PO: Membrane chaperone Shr3 assists in folding amino acid permeases preventing precocious ERAD. J Cell Biol. 2007, 176: 617-628. 10.1083/jcb.200612100.
  182. Kota J, Ljungdahl PO: Specialized membrane-localized chaperones prevent aggregation of polytopic proteins in the ER. J Cell Biol. 2005, 168: 79-88. 10.1083/jcb.200408106.
  183. Nagamori S, Smirnova IN, Kaback HR: Role of YidC in folding of polytopic membrane proteins. J Cell Biol. 2004, 165: 53-62. 10.1083/jcb.200402067.
  184. Ellgaard L, Molinari M, Helenius A: Setting the standards: quality control in the secretory pathway. Science. 1999, 286: 1882-1888. 10.1126/science.286.5446.1882.
  185. Casagrande R, Stern P, Diehn M, Shamu C, Osario M, Zuniga M, Brown PO, Ploegh H: Degradation of proteins from the ER of S. cerevisiae requires an intact unfolded protein response pathway. Mol Cell. 2000, 5: 729-735. 10.1016/S1097-2765(00)80251-8.
  186. Griffith DA, Delipala C, Leadsham J, Jarvis SM, Oesterhelt D: A novel yeast expression system for the overproduction of quality-controlled membrane proteins. FEBS Lett. 2003, 553: 45-50. 10.1016/S0014-5793(03)00952-9.
  187. Zhang Y, Nijbroek G, Sullivan ML, McCracken AA, Watkins SC, Michaelis S, Brodsky JL: Hsp70 molecular chaperone facilitates endoplasmic reticulum-associated protein degradation of cystic fibrosis transmembrane conductance regulator in yeast. Mol Biol Cell. 2001, 12: 1303-1314.
  188. Huyer G, Piluek WF, Fansler Z, Kreft SG, Hochstrasser M, Brodsky JL, Michaelis S: Distinct machinery is required in Saccharomyces cerevisiae for the endoplasmic reticulum-associated degradation of a multispanning membrane protein and a soluble luminal protein. J Biol Chem. 2004, 279: 38369-38378. 10.1074/jbc.M402468200.
  189. Vashist S, Ng DT: Misfolded proteins are sorted by a sequential checkpoint mechanism of ER quality control. J Cell Biol. 2004, 165: 41-52. 10.1083/jcb.200309132.
  190. Ravid T, Kreft SG, Hochstrasser M: Membrane and soluble substrates of the Doa10 ubiquitin ligase are degraded by distinct pathways. Embo J. 2006, 25: 533-543. 10.1038/sj.emboj.7600946.
  191. Nakatsukasa K, Huyer G, Michaelis S, Brodsky JL: Dissecting the ER-associated degradation of a misfolded polytopic membrane protein. Cell. 2008, 132: 101-112. 10.1016/j.cell.2007.11.023.
  192. Robinson NC, Zborowski J, Talbert LH: Cardiolipin-depleted bovine heart cytochrome c oxidase: binding stoichiometry and affinity for cardiolipin derivatives. Biochemistry. 1990, 29: 8962-8969. 10.1021/bi00490a012.
  193. Robinson NC: Specificity and binding affinity of phospholipids to the high-affinity cardiolipin sites of beef heart cytochrome c oxidase. Biochemistry. 1982, 21: 184-188. 10.1021/bi00530a031.
  194. Dudkina NV, Sunderhaus S, Boekema EJ, Braun HP: The higher level of organization of the oxidative phosphorylation system: mitochondrial supercomplexes. J Bioenerg Biomembr. 2008, 40: 419-424. 10.1007/s10863-008-9167-5.
  195. Figler RA, Omote H, Nakamoto RK, Al-Shawi MK: Use of chemical chaperones in the yeast Saccharomyces cerevisiae to enhance heterologous membrane protein expression: high-yield expression and purification of human P-glycoprotein. Arch Biochem Biophys. 2000, 376: 34-46. 10.1006/abbi.2000.1712.
  196. Murata Y, Watanabe T, Sato M, Momose Y, Nakahara T, Oka S, Iwahashi H: Dimethyl sulfoxide exposure facilitates phospholipid biosynthesis and cellular membrane proliferation in yeast cells. J Biol Chem. 2003, 278: 33185-33193. 10.1074/jbc.M300450200.
  197. Yu ZW, Quinn PJ: Dimethyl sulphoxide: a review of its applications in cell biology. Biosci Rep. 1994, 14: 259-281. 10.1007/BF01199051.
  198. Stimpson HE, Lewis MJ, Pelham HR: Transferrin receptor-like proteins control the degradation of a yeast metal transporter. Embo J. 2006, 25: 662-672. 10.1038/sj.emboj.7600984.
  199. Murakami K, Onoda Y, Kimura J, Yoshino M: Protection by histidine against oxidative inactivation of AMP deaminase in yeast. Biochem Mol Biol Int. 1997, 42: 1063-1069.
  200. Wagner S, Baars L, Ytterberg AJ, Klussmeier A, Wagner CS, Nord O, Nygren PA, van Wijk KJ, de Gier JW: Consequences of membrane protein overexpression in Escherichia coli. Mol Cell Proteomics. 2007, 6: 1527-1550. 10.1074/mcp.M600431-MCP200.
  201. Weiner JH, Lemire BD, Elmes ML, Bradley RD, Scraba DG: Overproduction of fumarate reductase in Escherichia coli induces a novel intracellular lipid-protein organelle. J Bacteriol. 1984, 158: 590-596.
  202. Jurgen B, Lin HY, Riemschneider S, Scharf C, Neubauer P, Schmid R, Hecker M, Schweder T: Monitoring of genes that respond to overproduction of an insoluble recombinant protein in Escherichia coli glucose-limited fed-batch fermentations. Biotechnol Bioeng. 2000, 70: 217-224. 10.1002/1097-0290(20001020)70:2<217::AID-BIT11>3.0.CO;2-W.
  203. Lesley SA, Graziano J, Cho CY, Knuth MW, Klock HE: Gene expression response to misfolded protein as a screen for soluble recombinant protein. Protein Eng. 2002, 15: 153-160. 10.1093/protein/15.2.153.
  204. Metzger MB, Michaelis S: Analysis of quality control substrates in distinct cellular compartments reveals a unique role for Rpn4p in tolerating misfolded membrane proteins. Mol Biol Cell. 2009, 20: 1006-1019. 10.1091/mbc.E08-02-0140.
  205. Mizuta K, Warner JR: Continued functioning of the secretory pathway is essential for ribosome synthesis. Mol Cell Biol. 1994, 14: 2493-2502.
  206. Bonander N, Darby RA, Grgic L, Bora N, Wen J, Brogna S, Poyner DR, O'Neill MA, Bill RM: Altering the ribosomal subunit ratio in yeast maximizes recombinant protein yield. Microb Cell Fact. 2009, 8: 10- 10.1186/1475-2859-8-10.
  207. Larschan E, Winston F: The S. cerevisiae SAGA complex functions in vivo as a coactivator for transcriptional activation by Gal4. Genes Dev. 2001, 15: 1946-1956. 10.1101/gad.911501.
  208. Heiland I, Erdmann R: Biogenesis of peroxisomes. Topogenesis of the peroxisomal membrane and matrix proteins. Febs J. 2005, 272: 2362-2372. 10.1111/j.1742-4658.2005.04690.x.
  209. Bolender N, Sickmann A, Wagner R, Meisinger C, Pfanner N: Multiple pathways for sorting mitochondrial precursor proteins. EMBO Rep. 2008, 9: 42-49. 10.1038/sj.embor.7401126.
  210. Hiller S, Garces RG, Malia TJ, Orekhov VY, Colombini M, Wagner G: Solution structure of the integral human membrane protein VDAC-1 in detergent micelles. Science. 2008, 321: 1206-1210. 10.1126/science.1161302.
  211. Bayrhuber M, Meins T, Habeck M, Becker S, Giller K, Villinger S, Vonrhein C, Griesinger C, Zweckstetter M, Zeth K: Structure of the human voltage-dependent anion channel. Proc Natl Acad Sci USA. 2008, 105: 15370-15375. 10.1073/pnas.0808115105.
  212. Ujwal R, Cascio D, Colletier JP, Faham S, Zhang J, Toro L, Ping P, Abramson J: The crystal structure of mouse VDAC1 at 2.3 A resolution reveals mechanistic insights into metabolite gating. Proc Natl Acad Sci USA. 2008, 105: 17742-17747. 10.1073/pnas.0809634105.
  213. Yang J, Ma YQ, Page RC, Misra S, Plow EF, Qin J: Structure of an integrin alphaIIb beta3 transmembrane-cytoplasmic heterocomplex provides insight into integrin activation. Proc Natl Acad Sci USA. 2009, 106: 17729-17734. 10.1073/pnas.0909589106.
  214. Stein A, Weber G, Wahl MC, Jahn R: Helical extension of the neuronal SNARE complex into the membrane. Nature. 2009, 460: 525-528.
  215. Gonzales EB, Kawate T, Gouaux E: Pore architecture and ion sites in acid-sensing ion channels and P2X receptors. Nature. 2009, 460: 599-604. 10.1038/nature08218.
  216. Kawate T, Michel JC, Birdsong WT, Gouaux E: Crystal structure of the ATP-gated P2X(4) ion channel in the closed state. Nature. 2009, 460: 592-598. 10.1038/nature08198.
  217. Maeda S, Nakagawa S, Suga M, Yamashita E, Oshima A, Fujiyoshi Y, Tsukihara T: Structure of the connexin 26 gap junction channel at 3.5 A resolution. Nature. 2009, 458: 597-602. 10.1038/nature07869.
  218. Jegerschold C, Pawelzik SC, Purhonen P, Bhakat P, Gheorghe KR, Gyobu N, Mitsuoka K, Morgenstern R, Jakobsson PJ, Hebert H: Structural basis for induced formation of the inflammatory mediator prostaglandin E2. Proc Natl Acad Sci USA. 2008, 105: 11110-11115. 10.1073/pnas.0802894105.
  219. Ferguson AD, McKeever BM, Xu S, Wisniewski D, Miller DK, Yamin TT, Spencer RH, Chu L, Ujjainwalla F, Cunningham BR, Evans JF, Becker JW: Crystal structure of inhibitor-bound human 5-lipoxygenase-activating protein. Science. 2007, 317: 510-512. 10.1126/science.1144346.
  220. Ago H, Kanaoka Y, Irikura D, Lam BK, Shimamura T, Austen KF, Miyano M: Crystal structure of a human membrane protein involved in cysteinyl leukotriene biosynthesis. Nature. 2007, 448: 609-612. 10.1038/nature05936.
  221. Teriete P, Franzin CM, Choi J, Marassi FM: Structure of the Na, K-ATPase regulatory protein FXYD1 in micelles. Biochemistry. 2007, 46: 6774-6783. 10.1021/bi700391b.
  222. Oxenoid K, Chou JJ: The structure of phospholamban pentamer reveals a channel-like architecture in membranes. Proc Natl Acad Sci USA. 2005, 102: 10870-10875. 10.1073/pnas.0504920102.
  223. Pedersen BP, Buch-Pedersen MJ, Morth JP, Palmgren MG, Nissen P: Crystal structure of the plasma membrane proton pump. Nature. 2007, 450: 1111-1114. 10.1038/nature06417.
  224. Bonander N, Bill RM: Relieving the first bottleneck in the drug discovery pipeline: using array technologies to rationalize membrane protein production. Expert Rev. Proteomics. 2009, 6: 501-505. 10.1586/epr.09.65.


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