Metabolic pathway engineering using the central signal processor PII
© Watzer et al. 2015
Received: 28 July 2015
Accepted: 6 November 2015
Published: 25 November 2015
PII signal processor proteins are wide spread in prokaryotes and plants where they control a multitude of anabolic reactions. Efficient overproduction of metabolites requires relaxing the tight cellular control circuits. Here we demonstrate that a single point mutation in the PII signaling protein from the cyanobacterium Synechocystis sp. PCC 6803 is sufficient to unlock the arginine pathway causing over accumulation of the biopolymer cyanophycin (multi-l-arginyl-poly-l-aspartate). This product is of biotechnological interest as a source of amino acids and polyaspartic acid. This work exemplifies a novel approach of pathway engineering by designing custom-tailored PII signaling proteins. Here, the engineered Synechocystis sp. PCC6803 strain with a PII-I86N mutation over-accumulated arginine through constitutive activation of the key enzyme N-acetylglutamate kinase (NAGK).
In the engineered strain BW86, in vivo NAGK activity was strongly increased and led to a more than tenfold higher arginine content than in the wild-type. As a consequence, strain BW86 accumulated up to 57 % cyanophycin per cell dry mass under the tested conditions, which is the highest yield of cyanophycin reported to date. Strain BW86 produced cyanophycin in a molecular mass range of 25 to >100 kDa; the wild-type produced the polymer in a range of 30 to >100 kDa.
The high yield and high molecular mass of cyanophycin produced by strain BW86 along with the low nutrient requirements of cyanobacteria make it a promising means for the biotechnological production of cyanophycin. This study furthermore demonstrates the feasibility of metabolic pathway engineering using the PII signaling protein, which occurs in numerous bacterial species.
KeywordsCyanophycin Cyanobacteria l-Arginine PII protein
Cyanophycin (multi-l-arginyl-poly-l-aspartate) is a nitrogen/carbon reserve polymer present in most cyanobacteria [1, 2] and in a few heterotrophic bacteria [3, 4]. It consists of a polyaspartic backbone with arginine residues linked via isopeptide bonds at the free carboxylate groups of the aspartic backbone [5, 6]. Cyanophycin is nonribosomally synthesized from arginine and aspartate by cyanophycinsynthetase (CphA) in an ATP-dependent elongation reaction using unidentified primers [6–8]. Cyanophycin accumulates in the cytoplasmic space as opaque, membrane-less granules . Isolated cyanophycin has a molecular weight widely ranging from 25 to 100 kDa  and is insoluble at physiological pH, but soluble in diluted acids or bases .
In cyanobacteria, the amount of cyanophycin is usually less than 1 % of the cell dry mass during exponential growth. When cells experience certain unfavorable conditions other than nitrogen starvation, such as stationary phase or unbalanced growth conditions owing to nutrient limitation, e.g., sulfate or phosphate starvation , light stress, low temperature , or presence of chloramphenicol , the cyanophycin content may increase to 18 % of the cell dry mass. Cyanophycin also can accumulate transiently during the recovery of nitrogen-starved, non-diazotrophic cyanobacteria upon addition of a usable nitrogen source . Furthermore, in heterocysts (specialized cells for nitrogen fixation) of cyanobacteria of the order Nostocales, polar nodules consisting of cyanophycin are deposited at the contact site to adjacent vegetative cells .
The cyanobacterial PII protein is a member of the widely distributed family of PII signal transduction proteins present in bacteria, plants, and some archaea . PII proteins are largely involved in the regulation of nitrogen assimilatory metabolism. For this purpose, PII senses the cellular energy level by binding ATP or ADP competitively  and senses the state of central carbon/nitrogen metabolism by binding or lack of binding of the status reporter molecule 2-oxoglutarate (2-OG) [18, 19]. Effector molecule binding results in structural rearrangements of the large surface-exposed T-loops of PII, its major protein-interaction determinant. In the unicellular freshwater cyanobacteria Synechococcus elongatus PCC 7942 and Synechocystis sp. PCC 6803 during nitrogen starvation, which corresponds with high 2-OG levels, the PII protein binds 2-OG and is phosphorylated at the apex of the T-loop at position Ser49; when nitrogen is in excess, which corresponds to 2-OG paucity and therefore no binding of the PII protein to 2-OG, Ser49 is dephosphorylated [16, 20].
Depending on the bound effector molecules and the phosphorylation status, PII interacts and influences many target proteins, including enzymes, channels, and regulatory proteins [18, 21, 22]. One of the major PII target proteins is the enzyme N-acetylglutamate kinase (NAGK) , which catalyzes the committed step in the cyclic arginine biosynthesis pathway . Under nitrogen excess, PII in its non-phosphorylated form binds to NAGK , there by strongly enhancing its biosynthetic activity as well as relieving the feedback inhibitory effect of arginine on NAGK activity . In a screening for PII variants with altered NAGK binding properties, our laboratory previously identified a variant of the S. elongatus PCC 7942 PII protein with a single amino acid replacement, Ile86 to Asp86, hereafter referred to as PII(I86N), that constitutively binds NAGK in vitro . The variant is a structural mimic of PII in the NAGK complex, with its T-loops in a kinked conformation; as a consequence of this special T-loop folding, this variant has a high affinity for NAGK and no longer responds to 2-OG but can bind citrate in vitro .
Results and discussion
Expression of the PII(I86N) variant in Synechocystis sp. PCC 6803 causes a strong in vivo activation of NAGK
Previous biochemical studies have shown that the PII(I86N) variant of S. elongatus PCC 7942 constitutively binds to NAGK in vitro . To test whether this PII variant affects the in vivo activity of NAGK, we constructed a genomic mutant of Synechocystis sp. PCC 6803 in which the glnB gene was replaced by a glnB gene carrying the mutation for I86N together with a spectinomycin resistance cassette via homologous recombination. Complete segregation of the mutation in the polyploidy Synechocystis sp. strain, named strain BW86, was confirmed via PCR (Additional file 1: Figure S1).
The PII(I86N) variant has a reduced phosphorylation
The high NAGK activity of the PII(I86N) variant leads to a high intracellular arginine level
The PII(I86N) mutation leads to cyanophycin accumulation
With ammonium as nitrogen source (Fig. 5b), wild-type cells accumulated cyanophycin similarly as with nitrate as nitrogen source, whereas strain BW86 produced less cyanophycin than in nitrate-supplemented medium, but still considerably more than the wild-type. The cyanophycin level increased up to 9.6 ± 1.7 % of the CDM in the first 4 days but began to slightly decrease on day 6. Quantification of the amount of ammonium in the medium supernatant of the two strains indicated that strain BW86 consumed ammonia more slowly than the wild-type (Additional file 2: Figure S2). In the first 2 days of cultivation, ammonia consumption of the wild-type and the BW86 strain was similar (Additional file 2: Figure S2). Subsequently, ammonia consumption in strain BW86 ceased. It is conceivable that the initial uptake of ammonium allowed initial cyanophycin accumulation, resulting in a peak of cyanophycin amount at day 2 and 4 (Fig. 5b). However, since after 4 days the strain BW86 stopped to consume ammonia and to grow (Fig. 5Bi), the cells might have degraded their cyanophycin reserves and used them as internal nitrogen source. The impaired ammonia consumption of strain BW86 could indicate a possible role of PII in ammonium utilization, which might be affected in the PII(I86N) variant. In Escherichia coli and many other heterotrophic bacteria, the PII homologue GlnK regulates the membrane-localized ammonia transporter AmtB . Although an involvement of cyanobacterial PII in the regulation of Amt homologues has not yet been clearly demonstrated, such a function seems possible . The phenotype of impaired ammonia utilization observed here could indicate a direct involvement of PII in ammonia uptake in Synechocystis sp. as well.
As nitrate-grown cells had higher cyanophycin contents than ammonium-grown cells, we used nitrate as the nitrogen source in the following studies. In some cyanobacterial species, the cyanophycin content can increase up to 18 % of the CDM [11–13, 31] under certain stress-conditions. Generally, cyanophycin accumulation is triggered by conditions of reduced growth rate, such as entry into stationary phase or unbalanced cultivation conditions, whereas during exponential growth, the amino acids arginine and aspartate are mostly used for protein biosynthesis. To test the effect of growth limitation on cyanophycin accumulation, we starved cells for phosphate or potassium (Fig. 5c, d, respectively).
To induce phosphate starvation cells were washed and inoculated in phosphate free BG-11 medium. Since the internal phosphate pools are only slowly depleted, the cell growth in phosphate free medium is initially not affected. In order to avoid growth into stationary phase without full induction of phosphate starvation, after 2 days, the cultures were again diluted 1:5 in phosphate free medium. After two more days, growth ceases due to phosphate starvation. Accordingly, the cyanophycin content of both strains on day 0 and day 2 (Fig. 5c) is comparable to that of non-starved cells (Fig. 5a). In agreement, the growth rate at this early stage was not affected because of a sufficient internal phosphate pool (Fig. 5Ci) . On day 4, the cyanophycin content in both the wild-type and strain BW86 strongly increased, correlating to the onset of the phosphate starvation. After 12 days, the accumulation of cyanophycin was maximal, with the wild-type exhibiting 16.2 ± 1.9 % of the CDM and strain BW86 47.4 ± 2.3 % of the CDM.
Potassium starvation is a very strong and immediate stress for cyanobacterial cells  because it is not buffered by internal pools and stringently affects the growth. In the absence of potassium, the growth rate of both strains was nearly zero  (Fig. 5Di). To test the effect of potassium starvation on cyanophycin production, exponentially growing cells of both strains were washed and inoculated into potassium-free BG-11 medium (Fig. 5d). In contrast to phosphate starvation, the cyanophycin content in potassium-starved cells rapidly increased in the first 2 days, due to the rapid arrest of growth. As long as the metabolism is in an active state, growth arrest allows the efficient synthesis of reserve materials. In agreement, cyanophycin accumulation in the wild-type reached a peak of 15.8 ± 0.5 % of the CDM after 4 days. In strain BW86, a peak of 57.3 ± 11.1 % cyanophycin per CDM was already reached on day 2. Thereafter, the cyanophycin content of both strains slowly decreased, probably a consequence of a stress response in the decaying cells, caused by the harmful lack of potassium.
Strain BW86 produces cyanophycin of high molecular mass
Microscopic examination of cyanophycin production in strain BW86
This work demonstrated the possibility of metabolic engineering using the PII(I86N) variant of the PII signal transduction protein to strongly increase arginine levels due to the PII dependence of the key enzyme of arginine biosynthesis, NAGK. As a consequence, cells of the engineered strain, strain BW86, overproduced arginine and over-accumulated cyanophycin of high molecular weight. This direct link further supports our previous assumption that cyanophycin synthesis is primarily controlled by cellular arginine levels . Taken together, the Synechocystis sp. strain described in this study, strain BW86, is the most potent cyanophycin producer described to date and is, therefore, a promising option for photoautotrophic production of arginine as well as cyanophycin. The large amount of cyanophycin of high molecular weight that can be produced with this strain opens the possibility of investigating novel applications of this polymer for biotechnological purposes.
In addition to the specific benefit of arginine and cyanophycin production obtained with the PII(I86N) variant, this study demonstrated the feasibility of using engineered variants of the PII signaling protein for metabolic engineering in bacteria. In addition to arginine synthesis, PII controls a multitude of other cellular activities in various autotrophic and heterotrophic bacteria. Therefore, metabolic pathways that are under control of this versatile regulatory protein could similarly be engineered.
Cultivation of bacteria
Standard cloning procedures were done in E. coli XL1-Blue (Stratagene) grown in Luria–Bertani medium at 37 °C with constant shaking at 300 rpm.
Cyanobacterial stains were grown photoautotrophically in BG-11 medium  containing nitrate or ammonium as nitrogen source and supplemented with 5 mM NaHCO3. Cultures were incubated in 50 or 200 ml medium in 100 or 500 ml Erlenmeyer flasks, respectively, at 28 °C with constant shaking at 120 rpm and illuminated with 50 µmol photons m−2 s−1. Larger cultures were grown in illuminated cylinders containing 800 ml medium supplemented with 5 mM NaHCO3, 5 mM TES/NaOH pH 8.2 (Roth). The cylinders were constantly aerated by bubbling 2 % CO2 in air through the liquid without additional shaking. Antibiotics were added to the media when required. Growth rates were monitored by measuring the optical density of the cultures at 750 nm.
Starvation conditions were induced by harvesting, washing, and transferring exponentially growing cells (OD750 0.4–0.5) into BG-11 media lacking a specific nutrient, i.e., no nitrogen source for nitrogen starvation; K2HPO4 replaced by KCl for phosphate starvation; and K2HPO4 replaced by Na2HPO4 for potassium starvation. In the case of phosphate starvation, after 2 days cultures were diluted again in phosphate-free BG-11 medium to an OD750 of 0.15 to avoid entry into stationary phase before cellular phosphate reserves were exhausted.
Construction of a PII(I86N)mutant
To construct a genomic PII(I86N) mutant of Synechocystis sp. PCC 6803, the PII-encoding gene glnB was genetically modified with the I86N mutation [Ile (5′ATC) at codon postion 86 to Asp (5′AAC)]. The entire cloning procedure is shown in Additional file 3: Figure S3. To incorporate the corresponding ATC to AAC mutation in the glnB gene, two amplicons of glnB were made using oligonucleotides PII(I86N)_rev (containing the ATC to AAC mutation) and PII_prom_for as well as PII_ter_rev (containing SacI restriction site) and PII(I86N)_for. Both glnB amplicons were fused by fusion PCR resulting in the mutated glnB amplicon. The genomic region downstream of glnB was amplified using slr0402_rev (containing NdeI restriction site) and slr0402_for primers. The mutated glnB amplicon was fused with the slr0402 fragment by fusion PCR and the resulting product was cloned in pJet 1.2 (Fermentas). Subsequently, a spectinomycin resistance cassette and a terminator sequence were inserted between the mutated glnB gene and the slr0402 fragment for later selection. A spectinomycin resistance cassette was first amplified using oligonucleotides spec r _for (containing SacI restriction site) and spec r _rev and was then fused with a terminator sequence that was, amplified using oligonucleotides Ter_rev (containing NdeI restriction site) and Ter_for. The product was inserted between the SacI and NdeI restriction sites of the glnB-slr0402 fusion product, resulting in pJet PII(I86N). See Additional file 4: Table S1 for a list of all oligonucleotides used to generate constructs.
Synechocystis sp. PCC 6803 was transformed with pJet PII(I86N) via natural competence ; transformants were selected on BG-11 agar plates supplemented with 25 µg/ml spectinomycin. Transformants were screened for complete segregation via PCR using oligonucleotides PII_prom_for and slr0402_for (Additional file 1: Figure S1).
In vivo NAGK activity assay
Cells (20 ml of a 50-ml culture at an OD750 of 0.8) were rapidly harvested by centrifugation and resuspended in a buffer consisting of 50 mM Tris/HCl pH 7.4, 4 mM EDTA, 1 mM DTT, and 0.5 mM benzamidine. Cells were lysed using FastPrep®-24 (MP biomedical) with 0.1 mm glass beads at a speed of 6.0 m/s for 20 s five times. The lysate was separated into soluble and insoluble fractions by centrifugation at 25,000×g for 25 min at 4 °C. The protein concentration of the soluble fraction was determined using the Bradford assay . NAGK activity of cell-free extract was measured according to Heinrich et al.  using 100 µg/ml protein for each measurement.
Determination of PII phosphorylation via western blotting
For non-denaturing electrophoretic separation of proteins, a native Gel was used according to Forchhammer et al. . Per lane, 10 µg of crude protein extract was loaded; after electrophoretic separation, the gel was blotted onto a PVDF membrane . The membrane was blocked with TBS blocking buffer (25 mM Tris/HCl pH 7.4, 75 mM NaCl) containing 1 % (v/v) Tween 20 overnight at 4 °C. The membrane was washed three times with TBS containing 0.1 % (v/v) Tween 20 (TBS-T) and afterwards incubated in TBS-T containing the anti-PII antibody  for 1 h at ambient temperature. Unbound antibody was removed by washing three times with TBS-T. Anti-rabbit IgG secondary antibody conjugated to horseradish peroxidase (α-rabbit polyclonal goat antibody, Sigma-Aldrich) diluted 1:10,000 in TBS-T was applied to the membrane and incubated for 30 min at ambient temperature. Unbound antibodies were removed by three washes with TBS-T. Bound antibodies were visualized using the Lumi Light detection system (Roche Diagnostics). Luminograms were taken with the Gel Logic 1500 imaging system (Kodak) with the associated software.
Metabolite extraction and quantification
For the extraction of metabolites, cells in 50 ml of culture at an OD750 of 0.8 were shock-cooled by mixing with crushed ice, rapidly harvested by centrifugation, and immediately frozen in liquid nitrogen. After freeze-drying, 5.0 mg lyophilized cells were homogenized with tungsten carbide beads in a Retsch Mill MM 200 (Retsch). Metabolites were extracted with 400 µl methanol, followed by a second extraction of the cells with 400 µl 20 % methanol with 0.1 % formic acid. The two supernatants were combined; solvents were removed using a vacuum concentrator. Metabolites were re-dissolved in 60 µl 20 % methanol with 0.1 % formic acid. A 5 µl aliquot was injected on a Waters UPLC/Synapt G2 LC/MS system equipped with a Waters Acquity 2.1 mm × 100 mm, 1.8 µm particle size HSS T3 reversed phase column. Metabolites were separated in a gradient from 20 % methanol with 0.1 % formic acid to 100 % methanol with 0.1 % formic acid in 10 min. The mass spectrometer was operated in ESI-positive and -negative modes with a scan range from m/z 50 to 2000 and a dwell time of 0.5 s. Data were evaluated using the MarkerLynx Software (Waters Cooperation, Milford, MA, USA) in combination with Simca-P (Umetrics AB Umea, Sweden). Compounds (based on formula and MSE fragmentation pattern) that differed between the different samples were identified by principal component analysis (PCA) and Orthogonal projections to latent structures (OPLS)—discriminant analysis (DA). From the entire metabolome, this procedure therefore identifies only those compounds, whose abundance differs between the two analyzed samples.
Cyanophycin extraction and quantification
Cyanophycin was extracted as described by Elbahloul et al.  with some modifications. Briefly, cells in 20–50 ml of culture at an OD750 of 0, 1–4 were harvested by centrifugation, resuspended in 100 % acetone, and incubated for 30 min with constant shaking at 1400 rpm. Cells were collected by centrifugation at 25,000×g for 15 min. The pellet was resuspended in 1.5 ml 0.1 M HCl and incubated for 1 h with constant shaking at 1400 rpm at 60 °C to solubilize cyanophycin. To remove debris, the sample was centrifuged at 25,000×g for 15 min. Cyanophycin in the clear supernatant was precipitated by adding 300 µl 1 M Tris/HCl pH 8.0 and incubating the mixture for 40 min at 4 °C. The mixture was then centrifuged at 25,000×g for 15 min at 4 °C. The supernatant was discarded, and the pelleted cyanophycin was dissolved in 500 µl 0.1 M HCl. Cyanophycin was quantified by determining arginine using the Sakaguchi reaction according to Messineo .
Cyanophycin isolation and determination of molecular mass
To determine the molecular mass of native cyanophycin, we modified the procedure of Ziegler et al.  to avoid hydrolyzation of cyanophycin by acid extraction. Cells were harvested and washed three times in buffer consisting of 50 mM Tris/HCl pH 7.4, 150 mM NaCl, and 5 mM EDTA. The cell pellet was resuspended in B-Per™ buffer supplemented with 100 µg/ml lysozyme and 5 U/ml DNase I. Cells were lysed using FastPrep®-24 (MP biomedical) with 0.1 mm glass beads at a speed of 6.0 m/s for 20 s five times. The lysate was separated into soluble and insoluble fractions by centrifugation at 25,000×g for 25 min at 4 °C. The insoluble fraction was washed three times with the same buffer and resuspended in B-Per™ buffer supplemented with 200 µg/ml proteinase K, which does not degrade cyanophycin, and incubated at 50 °C overnight. Cyanophycin granules were collected by centrifugation at 25,000×g for 25 min at 4 °C and washed three times with water. Cyanophycin was quantified as described above. To determine the molecular mass, cyanopycin granules were solubilized in SDS-loading buffer and separated by SDS-PAGE on a 12 % polyacrylamide gel according to Sambrook and Russell .
Microscopy and cyanophycin staining
Cyanophycin granules in bacterial cells were visualized microscopically using a newly developed staining method based on the Sakaguchi reaction. Cells of a 500 µl culture at an OD750 of 0.1–1.0 were collected via centrifugation and washed with 2.7 mM KCl, 1.5 mM KH2PO4, 137 mM NaCl, 8.1 mM Na2HPO4, pH 6.5 (PBS buffer). The cells were fixed by resuspending them in 500 µl PBS buffer containing 2.5 % (v/v) glutardialdehyde and incubated for 30 min at 4 °C. After fixation, the cells were washed with PBS and collected by centrifugation at 3000×g for 8 min at 4 °C. Then, cells were gently resuspended in 80 µl 5 M KOH and 10 µl of 1 % (w/v) 2,4-dichloro-1-naphthol dissolved in absolute ethanol was added; the mixture was incubated for 2 min at ambient temperature. Subsequently, 10 µl of 4–6 % (v/v) NaClO was added, and the mixture was incubated for 2 min. Finally, the cells were collected by centrifugation at 3000×g for 5 min, resuspended in 100 µl PBS buffer, and viewed under a Leica DM2500 microscope with a 100 ×/1.3 oil objective. Photographs were taken with a Leica DFC420C color camera.
Samples for transmissionelectron microscopy were prepared as described in Fiedler et al. . Briefly, samples were fixed and post-fixed using glutaraldehyde and potassium permanganate. The samples were embedded in EPON, and ultrathin sections were stained with uranyl acetate and lead citrate. The samples were examined with a Philips Tecnai electron microscope at 80 kV.
BW planned and performed experiments, analyzed and interpreted the data. AE and WH designed and generated stain BW86. MS performed the metabolomic study. IM performed the transmission electron microscopy. KF supervised the study, designed experiments and analyzed and interpreted the results. BW and KF wrote the manuscript. All authors read and approved the final manuscript.
This work was supported by the DFG-funded research training group GRK 1708 and by the “Cyanofood” program of the Ministerium für Wissenschaft, Forschung und Kunst Baden-Württemberg. We thank Alexander Klotz and Philipp Spät for help and general discussions. We thank Prof. Oliver Betz for providing TEM facilities, Claudia Menzel for technical assistance, Iris Stärk-Lenk for providing preliminary data, Karen Brune and Bernhard Watzer for carefully reading the paper.
The authors declare that they have no competing interests.
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