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To amplify DNA fragments for subsequent cloning, PCR with Phusion DNA polymerase was used. Components of PCR reaction are listed in Table 1.
All components of the PCR reaction were mixed on ice. PCR tubes with the reaction mix were transferred into a 98 °C preheated thermocycler and PCRs were performed according to the conditions listed in the Table 2.
Table 1 PCR reaction components and Table 2 PCR program.
All restriction enzymes used in our work were FastDigest enzymes from Thermo Fisher Scientific. Restriction reactions were prepared by mixing the following reagents (Table 3):
*FastAP (Thermosensitive Alkaline Phosphatase) was added to the vector restriction reaction in order to prevent self-ligation of the vector without the insert.
All components of restriction reactions were mixed in a 1.5 mL tube. After mixing, the restriction reaction was incubated at 37 °C for 30-60 min. Following the incubation, restriction enzymes were inactivated by heating the mixture for 15 min at 65-85 °C. As the next step, PCR clean-up protocol or gel electrophoresis followed by DNA purification from the gel was performed to clean the restricted DNA fragments.
Ingredients:
DNA was purified from the gel using the Gel-Out kit from A&A Biotechnology according to the manual instructions. A brief description of the procedure is written below. 1. DNA fragments of the correct sizes were cut out from the gel and transferred to Eppendorf tubes. 2. R7SI agarose melting solution was added; in case of < 2% agarose gel - 400 μL, in case of ≥ 2% agarose gel - 500 μL. Samples were incubated at 50°C until the complete dissolution of agarose slices. During incubation, the samples were mixed from time to time by inverting the tubes or vortexing. 3. An appropriate volume of Isopropanol was added. 4. < 2% agarose gel - 200 μL. 5. ≥ 2% agarose gel - 250 μL. 6. The samples were mixed by inverting the tubes. 7. After brief centrifugation, the mixture was transferred onto the minicolumns, which were centrifuged for 30 s at 10 000-15 000 RPM. 8. The flow-though was discarded and the minicolumns were re-assembled with the collection tubes. 9. At the next step, 600 μL of A1 wash solution were added and centrifugation for 30 s at 10 000-15 000 RPM was performed. 10. The filtrates were discarded and minicolumns were re-assembled with the collection tubes. 11. 300 μL of A1 wash solution were added. 12. Centrifugation for 1 min at 10 000-15 000 RPM was performed. 13. The dry minicolumns were transferred to the new 1.5 mL elution tubes and 50 μL of TE buffer were added directly onto the minicolumns resin. 14. Minicolumns were incubated for 3 min at room temperature and centrifuged for 60 s at 10 000-15 000 RPM. 15. The minicolumns were discarded. Purified DNA was used right away or kept at -20°C until needed. Additional protocols used:
DNA concentration measurements were carried out with NanoDrop Microvolume Spectrophotometer according to the manufacturer manuals. Software used: NanoDrop 1000 v.3.8.1. Mode used: Nucleic Acid, DNA-50
All ligation reactions were performed using T4 DNA ligase from NEB according to the manufacturer's instructions. All the components were mixed in a 1.5 mL tube in accordance with Table 4. DNA was taken using the 1:3 ratio of vector : insert based on the size of DNA fragments.
Table 4. Components of the ligation reaction.
Ligation reactions were kept at 16 °C for 2-4 hours or overnight (if ligation contains blunt ends). 1-2 µL of ligation mixture was used for bacterial transformation.
Golden Gate protocol was performed using the MoClo yeast kit developed by Lee et al. (2015). The kit includes a set of characterized parts which, together with custom-made parts, allow for assembly of synthetic constructs. The Golden Gate assembly reaction was mixed together based on Table 5 and the reaction program is shown in Table 6.
Table 5. Components of Golden Gate assembly reaction
Table 6. Golden Gate reaction Thermocycler program
Necessary components: Escherichia coli (E. Coli) competent cells Lysogeny Broth (LB) media
DNA transformation to bacteria cells was performed as follows:
Plasmids were extracted from bacterial cells using the “Plasmid Mini” kit by A&A Biotechnology according to manual instructions. A brief description of the procedure is written below.
Additional protocols used: FavorPrepTM Plasmid Extraction Mini Kit MonarchTM Plasmid Miniprep Kit
Plasmid extraction from yeast was performed following protocol written bellow:
STET buffer mentioned in this protocol was prepared according to such proportions:
In order to genetically transform yeast cells, the desired yeast strain was pre-grown in 50 mL of liquid YPD until OD600 0.6-0.8. The transformation was performed based on the following protocol:
Preparation of yeast cell lysates:
Preparation of PCR mixture
Components of the PCR reaction were mixed according to Table 7.
Table 7. PCR program.
Table 8.Components for PCR with “PCR Mix Plus Green” (Provided by A&A Biotechnology).
Conditions used for yeast colony PCR are described in Table 8.
Tables 9 and 10, respectively, provide list of components for preparation of LB and YPD media.
Table 9. YPD components.
Table 10. LB medium components.
Nile red is a lipophilic stain which can be used as a lipid droplet dye and can be visualized under a fluorescence microscope. Nile red staining was performed as described by Greenspan et al. (1985).
Ingredients: 1 mg/mL Nile red in DMSO Phosphate-buffered saline (PBS)
For the promoter characterization part, yeast colonies were checked after the transformation for the presence of GFP fluorescence. Prior to the experiment, yeast cultures were grown in synthetic complete uracil dropout medium with 2% glucose as a carbon source. The optical density (OD600) was in the range 0.2-0.6. Cultures were imaged under a Zeiss Axio Observer Z1 microscope. The following settings were used for the imaging: 25 ms exposure time for brightfield or phase-contrast, 100 ms exposure time for EGFP channel. Colibri LED modules were used as a source of 470 nm excitation at 25% intensity. Nile red was excited with the 470 nm LED for 5 ms. The fluorescence intensities were quantified using ImageJ.
Prior to time-lapse microscopy, the yeast cells were grown in synthetic complete (SC) media lacking histidine or SC lacking histidine and tryptophan depending on the integrative plasmids in the strain. The cultures were grown to OD600 0.2-0.8, the cells were pipetted onto a 0.08 mm cover glass slip and were covered with 1.5% agar-SC. Zeiss Observer Z1 microscope with 63C/1.4NA oil immersion objective and Axiocam 506 mono camera was used for imaging. The focus was kept using Definite Focus and the sample was kept at 30 °C using PeCon TempControl 37-2 digital. The cells were imaged every 5 minutes using brightfield illumination and the experiments were 13-18 hours long.
Plate readers are instruments that are used to detect samples in microtiter plates. We used BioTek Synergy MX microplate reader to measure the cells’ optical density and intensity of EGFP fluorescence. All strains used in the experiments were pre-grown overnight at 30 °C in liquid CSM/2%Glc media and diluted to OD600 in a range of 0.9 to 1.1. Then diluted cell cultures were distributed to 96 well plates (clear flat bottom). For replicates of two colonies from each strain were analyzed. 200 µL of cells were added to each well. CSM/2%Glc media was used as a reference to OD600. The measurements were done with the following parameters. Absorbance was measured at 600 nm and fluorescence was measured at the following conditions: excitation 485 nm, emission 528 nm, bandwidth 20, gain 80.
Ingredients: MQ water InP piece
Ingredients: MQ water FeCl3∙6H2O (5 mg mL-1) Tannic acid (40 mg mL-1) Tris-HCl buffer (pH 8.0, 1M) 70% ethanol
Ingredients: MQ water Polyallylamine hydrochloride (PAH) (5 mg mL-1)
Ingredients: FeCl3∙6H2O (5 mg mL-1) PBS (pH 7.4) MQ water
We used the Ellis Lab CRISPR/Cas9 toolkit as described by William Shaw. This method allows for markerless integration of multiple genetic cassettes into selected genomic loci. The toolkit consists of: An sgRNA entry vector A range of Cas9-sgRNA expression vectors Markerless integration cassettes
gRNAs targeting ACC1 region were designed using the Benchling CRISPR Guide RNA design tool. Four gRNAs with the highest on- and lowest off-target scores were chosen, and 5’ overhangs were added for cloning into a BsmBI-linearized plasmid. The following step describes the process of gRNA assembly and cloning.
Phosphorylation of oligos (inserts need to have 5’ phosphates for ligation, but synthesized primers do not have this).
The mixture was incubated 1h at 37 °C for phosphorylation reaction. Then PNK was inactivated at 75 °C for 10 min.
Once assembled and sequence verified, the sgRNA expression cassette was linearized with FastDigest Eco32I.
The mix was incubated at 37 °C for 30 min.
For genome editing, the following mix was prepared and used in the Super-High Efficiency yeast transformation protocol provided by Ellis Lab.
For transformation, we used 2 µL of the linearized Cas9-sgRNA repair vector (pWS171), 2 µL of linearized sgRNA cassette, and 36 µL of ACC1S686A S659A S1157A purified PCR product
The cultures were diluted to 106 cells/mL. Then, this culture was diluted 2, 10, 100 and 500 times. 5 µL of the dilution series was plated on YPD plates. The plated were incubated overnight at 30 °C.