Decrease of UPR- and ERAD-related proteins in Pichia pastoris during methanol-induced secretory insulin precursor production in controlled fed-batch cultures
© Vanz et al.; licensee BioMed Central Ltd. 2014
Received: 17 December 2013
Accepted: 7 February 2014
Published: 13 February 2014
Pichia pastoris is a popular yeast preferably employed for secretory protein production. Secretion is not always efficient and endoplasmic retention of proteins with aberrant folding properties, or when produced at exaggerated rates, can occur. In these cases production usually leads to an unfolded protein response (UPR) and the induction of the endoplasmic reticulum associated degradation (ERAD). P. pastoris is nowadays also an established host for secretory insulin precursor (IP) production, though little is known about the impact of IP production on the host cell physiology, in particular under industrially relevant production conditions. Here, we evaluate the cellular response to aox1 promoter-controlled, secretory IP production in controlled fed-batch processes using a proteome profiling approach.
Cells were first grown in a batch procedure using a defined medium with a high glycerol concentration. After glycerol depletion IP production was initiated by methanol addition which was kept constant through continuous methanol feeding. The most prominent changes of the intracellular proteome after the onset of methanol feeding were related to the enzymes of central carbon metabolism. In particular, the enzymes of the methanol dissimilatory pathway - virtually absent in the glycerol batch phase - dominated the proteome during the methanol fed-batch phase. Unexpectedly, a strong decrease of UPR and ERAD related proteins was also observed during methanol-induced IP production. Compared to non-producing control strains grown under identical conditions the UPR down-regulation was less pronounced indicating that IP production elicits a detectable but non prominent UPR response which is repressed by the general culture condition-dependent UPR down-regulation after the shift from glycerol to methanol.
The passage of IP through the secretory pathway using an optimized IP vector and growing the strain at fed-batch conditions with a high initial glycerol concentration does not impose a significant burden on the secretory machinery even under conditions leading to an extracellular accumulation of ~ 3 g L-1 IP. The glycerol batch pre-induction culture conditions are associated with a high constitutive - recombinant protein production independent - induction of the UPR and ERAD pathways probably preconditioning the cells for effective IP secretion in the methanol fed-batch phase.
The methylotrophic yeast Pichia pastoris is a well-established eukaryotic host for the production of heterologous proteins preferentially secreted into the medium to simplify further down-stream procedures [1, 2]. Secretory protein production usually requires the presence of a signal sequence at the N-terminus of the foreign protein to target it to the secretory pathway, namely allowing transfer of the protein into the endoplasmic reticulum (ER), passage through the Golgi apparatus, and, finally, vesicular transport to the extracellular environment. However, not all recombinant proteins are efficiently secreted and ER retention during high-level production can be a problem. In particular, aberrant folding properties of the target protein and/or high level production can lead to the accumulation of unfolded or even aggregated proteins in the ER [3–6] which can initiate the unfolded protein response (UPR) [5–10] and ER-associated degradation (ERAD) [5–7].
Simplified, overloading of the secretory pathway is sensed in the ER by binding of KAR2 (or BiP) to folding intermediates or misfolded proteins which outcompete the binding of KAR2 to the ER luminal domain of IRE1 [11–13]. The release of KAR2 from the luminal IRE1 domain leads to conformational changes and autophosphorylation and subsequent activation of the cytosolic IRE1 endoribonuclease domain. This leads to splicing of the IRE1 substrate, HAC1 mRNA, being transformed into the activated form encoding the transcriptional activator of UPR responsive genes, Hac1p [11–13].
Many UPR responsive genes encode ER resident chaperones and foldases, including the most prominent ER chaperone, KAR2, and the major ER disulfide isomerise, PDI. In addition to acting as the sensor protein for the presence of un-/misfolded proteins, KAR2 is also involved in chaperoning protein folding thereby relieving from protein (mis) folding associated stress in the ER . PDI is responsible for disulfide exchange reactions in the ER helping to rearrange incorrect disulfide pairings . Both proteins as well as Hac1(p) have been co-overproduced in P. pastoris for enhanced secretion of target proteins with mostly unpredictable and varied success [3, 12, 16–20].
The induction of the UPR response in P. pastoris through recombinant protein production was mainly studied using a transcriptome based approach [5, 6, 8–10, 21]. In all these cases transcript or transcriptome analysis revealed enhanced expression of UPR-related genes during secretory recombinant protein overproduction [5, 8–10] or ERAD-related genes in case of a high propensity of the recombinant protein to misfolding an/or retention in the ER [5, 6]. Moreover, UPR induction was also detected by increasing levels of KAR2 (protein) upon secretory recombinant protein overproduction [22, 23]. Recently, also more comprehensive proteomic studies were carried out to monitor the induction of the UPR and other stress responses during recombinant protein production in P. pastoris[7, 19]. These studies revealed increased levels of UPR related proteins upon methanol induced production of secretory xylanase  and ER residing Hepatitis B surface antigen . However, only the production of the Hepatitis B surface antigen, a protein retained in the ER , also led to an ERAD response apparent through the strong increase of two cytosolic chaperones and members of the AAA ATPase superfamily which are participating in ERAD . No ERAD response was observed during secretory xylanase production . UPR and ERAD are coordinated responses in yeast as has been shown in more detail for Saccharomyces cerevisiae, however, a strong ERAD response might only be necessary if the ER cannot get cleared by a regular and coordinated passage of the target protein through the entire secretory pathway.
In this study we have analyzed the cellular response towards methanol induced secretory insulin precursor (IP) production with special attention to the occurrence of proteins related to the UPR and ERAD pathways. Surprisingly, our analysis revealed a decrease of UPR and ERAD related proteins in response to secretory IP production under industrially relevant production conditions.
Results and discussion
A proteome profiling approach was chosen to evaluate the cellular response of P. pastoris towards secretory IP production under industrially relevant production conditions. The recombinant strain was first grown to high-cell density in a batch procedure using a defined medium with low salt and high glycerol concentrations . After depletion of glycerol, secretory IP production was induced by methanol addition to a final concentration of 2 g L-1 which were kept constant by continuous methanol feeding leading to final extracellular IP concentrations of ~ 3 gram per liter of culture broth  with less than 10% IP remaining intracellular (data not shown). The details of the original cultivation data are given elsewhere  and the list of all identified proteins is shown in the Additional file 1: Table S1.
General proteomic response towards methanol-induced secretory IP production in controlled fed-batch culture
UPR and ERAD responses during secretory IP production in controlled fed-batch culture
Despite the high-level secretory production of a foreign protein, UPR and ERAD related proteins strongly decreased in the IP producing strain during the methanol fed-batch phase (Figures 1, 2, 3, Additional file 1: Figures S1 and S2, and Additional file 1: Table S2). A significant decline of many UPR-related proteins became already apparent 18 hours after the onset of methanol feeding (Figure 2). This included the most prominent chaperone of the ER, KAR2 (also known as BiP) which decreased to almost undetectable levels (Figure 2 and Additional file 1: Figure S2). In addition to the typical ER resident chaperones and foldases (e.g. KAR2, PDI) also cytosolic and mitochondrial chaperones decreased in abundance during the methanol fed-batch phase (Figures 2, 3, Additional file 1: Figures S1 and S2, and Additional file 1: Table S2). For example, the identified cytosolic chaperones with decreasing abundance, e.g. members of the HSP70 family (SSA1, SSA3 and SSB) are encoded by UPR-responsive genes which show increased expression in Hac1p overproducing strains . Moreover, two cytosolic chaperones and members of the AAA ATPase superfamily (ClpB = HSP104 and the AAA ATPase PAS_FragD_0026 = CDC48) also decreased strongly in abundance during the methanol fed-batch phase (Figures 2, 3, Additional file 1: Figures S1 and S2, Additional file 1: Table S2). Both proteins are members of the ERAD pathway which ultimately target misfolded proteins from the ER to cytosolic proteasomal degradation . For example, the AAA ATPase CDC48 is a ubiquitin-binding protein engaged in the delivery of multi-ubiquitinated proteins to the proteasome for final degradation [27, 28]. In this line, the ubiquitin activating enzyme UBA1, which catalyses the first step in ubiquitination  also decreased in abundance after the shift from the glycerol batch to the methanol fed-batch phase (Figures 2, 3, Additional file 1: Figures S1 and S2, and Additional file 1: Table S2). The mitochondrial chaperones CPNA (HSP60 family) and SSC1 (HSP70 family) which also revealed a decreasing abundance in the methanol fed-batch phase are not directly involved in recombinant (secretory) protein folding and degradation, but are classical UPR targets induced by HAC1 overexpression or dithiotreitol addition . The observed decrease of UPR and ERAD related proteins in the methanol fed-batch phase strongly suggests that other non-recombinant protein related effects might be responsible for their observed decline during IP production. Moreover, the low increase of biomass during the production phase  also suggests that the restructuring of the intracellular proteome after growth on glycerol to methanol induced IP production results from de- and reconstruction processes and not simply from dilution and de novo synthesis.
UPR response in host (control) and IP producing strains at different methanol concentrations in shake flask culture
During methanol-induced secretory IP production a general decrease of UPR and ERAD related proteins occurred within P. pastoris at the culture conditions employed. Compared to the non-producing host strain the UPR down-regulation was less pronounced indicating that production of IP elicits a detectable but non prominent UPR response which is repressed by a general culture condition dependent UPR down-regulation after the shift from glycerol to methanol. Appearance and removal of misfolded proteins are inherent incidents during normal growth  which might be differently regulated at different environmental conditions. Previous findings indicated that the extend of the UPR in yeast is also connected to the nutritional state of the cell  and, as has been shown for P. pastoris, also to other environmental conditions such as osmolarity  and temperature . Environmental factors are presumably responsible for the high level of UPR and ERAD related proteins in the batch phase in which high concentrations of glycerol were employed. Moreover, there are also - though not yet conclusive - indications that P. pastoris may exhibit in general a stronger constitutive or basal induction of the UPR as other yeast independent of the production of aberrant proteins [6, 12, 13]. Our findings also indicate that IP is a quite stable protein as it has been shown that the native-state stability of a secreted protein is inversely correlated to its UPR and ERAD inducing effect . Thus, the properties of IP, e.g. its stability as well as the moderate induction conditions do not provoke significant folding stress during IP production in the controlled fed-batch process. Above all, the high levels of UPR related proteins prior to induction probably precondition the cells for effective IP secretion in the methanol induction phase and this “more constitutive” UPR induction might be responsible for the superior secretion properties of P. pastoris.
Materials and methods
Strains and growth conditions
The P. pastoris host strains X-33 and GS115 were from Invitrogen (Carlsbad, CA, USA). Details of the construction of the recombinant P. pastoris strain X-33 carrying a codon-optimized copy of a synthetic IP gene for secretory IP production under the control of the aox1 promoter (Mut+) and usage of the α-factor secretory signal are given elsewhere .
Bioreactor fed-batch cultivations
Growth and insulin precursor production under industrially relevant conditions using a defined medium were essentially carried out as described before . Cells were first grown in a batch procedure using glycerol as sole carbon source with an initial glycerol concentration of 95 g L-1[25, 26]. After depletion of glycerol, insulin precursor production was induced by a pulsed methanol addition and subsequent methanol feeding to maintain the methanol concentration at 2 g L-1. Initially, the methanol concentration was increased in a step-wise manner to the final concentration of 2 g L-1 but in follow-up cultivations the methanol concentrations were immediately increased to 2 g L-1 without detectable effects on the final product yield and cell responses (see also Additional file 1: Figure S2).
Shake flask cultivations
500 mL baffled shake flasks containing 100 mL basal medium (20 g L-1 glycerol, 13.4 g L-1 yeast nitrogen base without amino acids, 400 μg L-1 biotin in ddH2O) were inoculated from glycerol stocks. The cultures were grown for approximately 36 h at 30°C and 250 rpm to an OD600 8–10 and used to inoculate the next preculture (1% inoculum, 100 mL basal medium). This preculture was grown for approximately 20 h (OD600 3–5) and taken as an inoculum for the main culture (10% inoculum, 450 mL defined medium, 2 L baffled shake flasks). The defined medium was identical to the medium employed for the glycerol batch phase in bioreactor cultures [25, 26]. The main cultures were grown for 30–40 h at 30°C and 150 rpm, the cells collected by centrifugation, washed with sterile PBS and resuspended in defined medium without glycerol to OD600 100. Recombinant protein production was induced by the addition of 1% or 2% methanol (every 12 h repeated).
Sample preparation for two-dimensional gel electrophoresis, two-dimensional gel electrophoresis, and protein spot identification and quantification
All procedures were carried out essentially as described previously . After harvesting by centrifugation, cell pellets were immediately flash-frozen in liquid nitrogen and kept at −80°C before further treatments.
Cell pellets were washed with ice-cold phosphate-buffered saline (PBS), resuspended in 1 mL cell lysis buffer (7 mol L-1 urea, 2 mol L-1 thiourea, 4% (w/v) Triton X-100, 30 mmol L-1 Tris, pH 8.5) with the OD600 adjusted to OD 50 and combined with 500 μL of glass beads (0.5 mm, Sartorius, Germany). For cell disruption, samples were treated twice in a Thermo Savant Fastprep FP120 homogenizer (speed 6.00 m/s for 30 s; cooling interval of 30 s between treatments). Following, cell debris was removed by centrifugation at 13000 rpm and 4°C for 5 min and proteins in the supernatant precipitated using chloroform and methanol. The protein pellets were air-dried and dissolved in 500 μL of resolubilization solution (9 mol L-1 urea, 2 mol L-1 thiourea, 4% CHAPS, 2 mg mL-1 Tris, 0.2% SDS, 0.002% bromophenol blue). To this solution, 7.5 μL IPG buffer (Amersham Biosciences, UK) and 7.5 μL 1 mol L-1 dithiothreitol were added and the resolubilized proteins stored at -80°C until further analysis.
Two-dimensional gel electrophoresis
The first-dimension of isoelectric focussing (IEF) was carried out using the IPGphor™ Isoelectric Focussing System (Amersham Biosciences, UK) at 20°C with a current of 30 μA per strip. 400 μg of each protein sample were loaded onto Immobiline DryStrip gels of pH 3–10 NL (Amersham Biosciences, UK) by in-gel rehydration. IEF was performed with the following setting: 0 V × 35 h, 50 V × 4 h, gradient from 100 V to 300 V within 4 h, gradient from 300 V to 1000 V within 3 h, gradient from 1000 V to 3500 V within 4 h, gradient from 3500 V to 5000 V within 3 h, 5000 V × 3 h, gradient from 5000 V to 8000 V within 3 h, then 8000 V × 10 h. The second-dimension was carried out using 12% SDS-PAGE gels and the vertical separation unit Hoefer™ System (Amersham Biosciences) at 10°C in constant working voltage mode as follows: 40 V for 2 h and then 100 V overnight. Subsequently, gels were stained using colloidal Coomassie Brilliant Blue G-250 according to the “Blue silver” protocol . The gels were then scanned (Epson Perfection V750 Pro, Epson, Germany) at 300 dpi resolution to acquire the gel images.
In-gel trypsin digestion and peptide extraction
Protein spots were excised manually from the stained gels, washed several times with 200 μL water, dehydrated in 200 μl acetonitrile, and dried in a vacuum concentrator (Eppendorf® Vacufuge Concentrator 5301, Eppendorf AG, Hamburg). The gel pieces were treated with 100 mmol L-1 ammonium bicarbonate, containing 20 mmol L-1 DTT at 56°C for 30 min and then with 100 mmol L-1 ammonium bicarbonate containing 55 mmol L-1 iodoacetamide in the dark at room temperature for 30 min. Acetonitrile was added in between the treatments to dehydrate the gel pieces. Finally, the gel pieces were washed twice with 100 mmol L-1 ammonium bicarbonate, dehydrated with acetonitrile and dried in the vacuum concentrator. In-gel digestion was carried out by incubation with 2 ng μL-1 trypsin (sequencing grade modified, Promega Corp., USA) in 50 mmol L-1 ammonium bicarbonate at 37°C overnight. Obtained peptides were extracted, washed with a buffer for desalting (10 mmol L-1 ammonium phosphate, monobasic in 0.1% trifluoroacetic acid (TFA) and then loaded to a Prespotted Anchor Chip (Bruker Daltonics GmbH, Germany) targeted for MALDI-TOF analysis. The molecular masses of the tryptic peptides were determined on a Bruker Ultraflex time-of-flight mass spectrometer (Bruker Daltonics GmbH, Germany).
Protein identification and quantification
Peptide mass fingerprints obtained by the MALDI-TOF MS were processed using FlexAnalysis 2.0 (Bruker Daltonics GmbH, Germany) and used to search the NCBInr database by using Mascot 2.10 software (http://www.matrixscience.com). The parameters used for searching were as follows: taxonomy: other Fungi, tryptic digestion, modifications were allowed for carbamidomethylation of cysteine (fixed modification) and methionine oxidation (variable modification), one missed cleavage site was allowed, all peptides monoisotopic, peptide tolerance at 100 ppm. Mascot scores (probability based MOWSE scores) and expect values were generated using the Mascot search program. All proteins with a Mowse score greater than 71 were regarded as significant (p < 0.05). For most peptide mass fingerprints, a single significant hit (P < 0.05) with a probability-based Mowse score greater than 71 was obtained. In rare cases the Mowse score was below 71, which indicated that the protein was not identified with reliability above the level of significance. These protein spots were excluded from the results unless the identification was confirmed by MS/MS. Image analysis from the scanned gels, namely protein spot detection, matching and quantification were performed using Proteomweaver™ 3.0 (Definiens AG, Germany). For each sample, 2D gels were made in triplicate. And the best two gels were analyzed. The spot volumes were computed and normalized for each spot on each gel in relation to the total spot volume of each 2D gel. To obtain comparable data, spot intensities were normalized, using the log2 ratio of induced samples versus uninduced samples. Log2 fold changes above 0.6 (equivalent to a 1.5 fold change) were considered significant. The gene name used is this study is according to P. pastoris strain GS115 (http://www.uniprot.org/). If no gene name is given for this strain the gene name is according to P. pastoris strains (ATCC 76273/CBS 7435/CECT 11047/NRRL Y-11430/Wegner 21–1) or P. pastoris (yeast) in case of 100% sequence identity (http://www.uniprot.org/).
Cells were collected by centrifugation and resuspended in lysis buffer (5 mmol L-1 EDTA, 0.5 mol L-1 NaCl, 8% glycerol, 1 μg/mL pepstatin A, 1 mmol L-1 PMSF, 25 mmol L-1 phosphate buffer, pH 8.0) corresponding to a suspension of 700 μL (OD600 30). For cell disruption, this suspension was combined with 500 μL of glass beads (0.5 mm, Sartorius, Germany) and treated seven times in a Thermo Savant Fastprep FP120 homogenizer (speed 6.00 m/s for 30 s; cooling interval of 30 s between treatments).
Western blotting and immunostaining
Proteins were separated on 12% SDS-PAGE gels prior to electroblotting onto PVDF membranes (Bio-Rad, Hercules, USA) at 12 volts for 45 min. On each lane, the same sample volume was loaded corresponding to an identical OD600. The membranes were blocked with 5% skimmed milk (Difco, France) in PBS containing 0.5% Tween 20 (PBS-T) for 2 h. After washing the membranes with PBS-T, the mouse anti-HDEL antibody (2E7) (sc-53472; 1:1000 dilution, Santa Cruz Biotechnology, USA) was added and the membranes incubated for 1 h at room temperature. After washing with PBS-T, the secondary anti-mouse antibody (1:5000 dilution, Calbiochem, Germany) was added and incubation continued for 1 h. Immunostaining was done using 3,3’,5,5’ tetramethylbenzidine (Sigma, Germany) as substrate. The mouse anti-HDEL antibody (2E7) binds only to the six P. pastoris proteins containing the C-terminal HDEL sequence, namely KRE5 (166.2 kDa), SEC12 (116.2 kDa), LHS1 (99.5 kDa), KAR2 (74.2 kDa), PDI1 (57.8 kDa), and MPD1(33.5 kDa) .
Ana Letícia Vanz would like to acknowledge the Federal Agency for the Improvement of Higher Education, Brazil (CAPES) for providing a PhD fellowship. We are also grateful to Anja Meier for skilful support in MS sample preparations.
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