Difference between revisions of "Team:LMU-TUM Munich/Methods"

For transformation of E. coli XL-1 blue chemically competent cells, cells were thawed on ice for 5 mins. 50-100 ng plasmid DNA (or ~200 ng ligation product) were added, and cells were further incubated on ice for 20-30 mins. Afterwards, a heatshock was applied at 42°C for 45 secs. Cells were then further incubated on ice for 2 mins, and 950 μl of LB medium were added. Cells were then shaken at 200 rpm for at least 1 h at 37°C, and plated on LB-agar plates containing the appropriate antibiotic. The next day, single clones were picked and used to inoculate a liquid culture of 5 ml LB medium. After being incubated overnight shaking (200 rpm) at 37°C, cells were spun down (6000 g, 5 mins), and plasmid DNA was extracted using the Qiagen QIAprep Spin Miniprep Kit. If ligation products were used for transformation, analytical digestion of DNA was performed to confirm the correct incorporation of the desired fragment. Therefore, DNA was digested with ~0.5 U suitable restriction enyzmes for 1 h at 37°C and analyzed via analytical gel electrophoresis. Additionally, plasmids were sequenced using the Eurofins Genomics sequencing service.

DNA concentrations were determined spectrophotometrically using a Nanodrop device. From the measured absorption at 260 nm, DNA concentrations were determined, an absorption of 1 being equal to a concentration 50 ng/μl DNA. Furthermore, wavelengths at 280 nm and 230 nm were measured to confirm sample purity without contamination of proteins (280 nm) or carbohydrates, phenol or EDTA (230 nm). Ratios of 260/280 nm being in the range between 1.6 and 2.0, as well as the ratios of 260/230 nm being between 2.0 and 2.2 generally indicate sample purity.

For cloning, DNA was digested using restriction endonucleases. The amount of used enzyme hereby depended on the amount of to be digested DNA, whereas ~1 unit was used per μg of DNA. Buffers and DNA concentrations were used according to the manufacturer's suggestion. Digestions were incubated at 37°C. If deemed necessary, 5’-ends of vector fragments were dephosphorylated for 30 min at 37 °C directly by addition of alkaline phosphatase (Fast-AP) to the restriction mixture at 37°C, incubation for 10 mins and inactivation of the enzyme for 5 mins at 75°C.

Ligations were conducted using the appropriate DNA fragments while adding 400 units of ligase in the appropriate buffer. Vector and insert fragments were generally used at a 1:3 ratio, while the amount of vector fragment DNA was varied between 50-100 ng.

For separation of DNA fragments, agarose gel electrophoresis was used. For fragments with a size of more than 500 bp, 1% (m/V) agarose gels were used. For smaller fragments, agarose concentration was increased as deemed necessary, until concentrations of up to 1.8% (m/V) agarose. For the production of gels, the appropriate amount of agarose was solved in 50 ml TAE buffer by heating the suspension. For staining, ethidium bromide was added into the mixture. Gels were run at 100 V for analytical and at 80 V for preparative use (200 mA respectively). For preparative gels, DNA fragments were excised and extracted from the gel using the Qiagen Gel Extraction Kit according to the manufacturer's protocol.

For the amplification of DNA fragments, polymerase chain reaction was conducted. Hereby, 50 µl PCR mixture contained 50-500 ng template DNA, 100 pmol of each primer, and 10 nmol of each desoxynucleotide (dATP, dCTP, dGTP, dTTP). Additionally, the mixture contained 1 U Q5 high-fidelity polymerase and Q5 polymerase buffer, and was filled up with ddH₂O to the final volume. For the PCR, double-stranded fragments were initially denaturated at 98 °C for 2 min and subsequently amplified in 25-30 repetitive cycles, each comprising three steps: (1) Denaturation of the double-stranded DNA (98 °C, 30 s), (2) annealing of the primer to the single-stranded template for 30 s at 50-65 °C (depending on the melting temperature of the primer-template hybrid), and (3) extension of the primed DNA template (72 °C, 60 s per kb fragment length). After that, a final elongation step (2 min, 72 °C) was included to ensure that remaining single-stranded template molecules are fully elongated.

Then, the PCR product was separated by agarose gel electrophoresis to check for its correct size and isolated from the gel as described or directly isolated from the PCR reaction mixture, respectively using the Qiagen Gel extraction and PCR purification kit.

The anti-PDGF ELISA was done using the abcam 'ab184860 - PDGF BB Human SimpleStep ELISA® Kit'. In short, this kit provides a 96-well plate that is already coated with anti-PDGF antibodies, which are then coupled with a further primary and secondary antibody. For measurements, 20 μl of the medium taken at the respective measurements were diluted with 80 μl sample dilution buffer. Then, a dilution series was made that diluted the mixture three times by a factor of 8 with sample dilution buffer, to a total number of four wells per sample. Wells were then washed three times with washing buffer, detection substrate was added and the mixture incubated for 1 h at RT at 400 rpm. Afterwards, stop-buffer was added and an end-point absorption measurement at 450 nm was made.

A frozen glycerol stock of the desired strain of E. coli cells was streaked out on a LB plate under sterile conditions and incubated overnight at 37°C. A 4 ml LB medium liquid preculture was then inoculated and incubated overnight at 37°C shaking. 500 μl starter culture were used to inoculate a 50 ml LB medium liquid culture. When reaching an OD₆₀₀ of 0.45-0.5, the culture was immediately chilled on ice for 10 mins, and harvested by centrifugation at 3000g for 10 mins at 4°C. The supernatant was cast away, and the pellet resuspended in 40 ml of ice cold 100 mM MgCl₂. Cells were spun down again at 3000 g for 10 mins at 4°C, and the pellet resuspended in 20 ml of ice cold 50 mM CaCl₂. This suspension was kept on ice for 30 mins, and harvested by centrifugation at 3000 g for 10 mis at 4°C. The pellet was resuspended in 2 ml ice cold 50 mM CaCl₂ and 15% glycerol. The resulting bacterial suspension was sampled in 1.5 ml microcentrifuge tubes, frozen in liquid nitrogen and stored at -80°C until further use.

Protein concentrations were determined via UV/VIS spectrometry. According to Lambert-Beer’s law, the measured absorption at 280 nm (0.1 < A₂₈₀ < 1) was normalised by the extinction coefficient of the protein, which can be predicted by ProtParam based on its sequence. Considering the given dilution and the length d of the cuvette, a protein concentration can be predicted by c = A₂₈₀/(ε*d)

Ion exchange chromatography is based on the separation of proteins with different electrostatic properties (pI values) by binding them on a charged matrix and their displacement and elution via a salt gradient. Positively charged proteins (pH < pI) can be separated by cation exchange chromatography using a Resource Q column (Quaternary ammonium). Negatively charged proteins (pH > pI) in contrast, are purified with a Resource S column (Sulphonate group).
Columns being used are Res S and Res Q and have a volume of 6 ml.

Size exclusion chromatography is a chromatographic method based on different diffusion times of proteins through a gel matrix in dependence on the hydrodynamic radius of the target protein; heavier proteins generally eluting earlier due to higher diffusion speeds through the gel matrix.

If a target protein is expressed as a SUMO/TEV peptide fusion construct with His₆-tag, the recombinantly expressed protein could be purified via IMAC. IMAC makes use of the interaction of imidazole side chains of histidine residues with immobilised nickel ions. Using this method, the target protein can be eluated by addition of imidazole, which competitively binds to the column and thus displaces the target protein in the column, causing it to eluate.

After harvesting cells the target protein was purified using a stripped and equilibrated HiTrap IMAC HP column (6 ml volume). Therefore, the column was loaded with the sample and washed with buffer A until absorption at 280 nm hit zero. For elution, a -linear/step- imidazole gradient was set. The resulting fractions were analysed by SDS-polyacrylamide gel electrophoresis and were pooled for further purification, if their purity was deemed sufficient. In order to remove imidazole, dialysis was conducted overnight, using 5 l dialysis buffer.

For size exclusion chromatography of the streptavidin variants, 0.5 ml of concentrate was loaded on a Sephacryl S300 16 60 column. Resulting peak fractions were respectively loaded onto an SDS-gel. Possible Streptavidin aggragates and monomers were removed, fractions of the tetramer were pooled.

For analysis of recombinant protein expression, discontinuous SDS-polyacrylamide gel electrophoresis was conducted. Therefore, samples were mixed with Laemmli buffer (finalc concentration 1x) and incubated at 95°C for 5 min. For electrophoresis, currents of 60 mA were used, while voltage was initially set to 90 V and raised to 130 V after 10 mins. For staining, the gel was incubated with Coomassie brilliant blue R250 in H2O:MeOH:HAc (5:4:1) for 30 minutes.

The minimal Streptavidin wildtype gene is cloned on a pSA plasmid. The transcription is under control of a T7-promoter. The E.coli BL-R (DE3) strain codes the T7-polymerase under the control of a lacUV5 promotor, which can be induced by Isopropyl β-D-1-thiogalactopyranoside (IPTG). A shaking flask with 2 L LB medium supplemented with ampicillin is inoculated 1:40 with a 50 ml preculture grown at 30 °C over night. The bacterial culture shakes at 37 °C for a few hours until its optical density reaches 0.6 and protein production is induced with 1 mM IPTG. After 4 hours the cells can be harvested by centrifugation (5000 rpm for 20 min). The cell pellet is resuspended in a 20 mM Tris/HCl buffer (500 mM NaCl, pH 8) and Homogenization can be proceeded with French press or PANDA. The cell lysate is centrifuged at 11500 rpm for 30 min to separate the inclusion bodies in the pellet from the soluble proteins of the supernatant. The inclusion bodies consist of aggregated and misfolded protein, those are denaturated with 6 M guanidinium chloride and centrifuged at 15000 rpm for 15 minutes. The aggregations in the pellet are discarded and the supernatant is added slowly into a high volume of PBS (30 ml PBS for 1 ml protein solution) and incubated over night. Guanidinium chloride is diluted and proteins are able to fold correctly.The solution is centrifuged again (11500 rpm for 30 min) to remove aggregates. The Streptavidin purification is proceeded by fractionally ammonium sulfate precipitation. After each precipitation step the solution is incubated without stirring for few hours and centrifuged at 11500 rpm for 30 minutes afterwards. The first precipitation step is 40 % saturation (1.75 M). Streptavidin remains soluble, the pellet can be discarded. After centrifugation the ammonium sulfate saturation is increased up to 70 % (3.37 M), Streptavidin is no longer soluble and precipitates. The pellet is resuspended in a 50 % saturated ammonium sulfate solution (2.25 M), streptavidin again precipitates. After centrifugation the pellet is resuspended in 1x PBS buffer. As a result the solution contains only those proteins, which precipitate between 40 % and 50 % ammonium sulfate saturation. One last centrifugation at 15000 rpm for 30 minutes removes insoluble impurities. The solution is dialysed against 20 mM Tris/HCl buffer without salt (pH 8). Streptavidin has an isoelectric point of 6.09, therefore it is negatively charged in its buffer and a positively charged ResQ column is used for ion exchange chromatography. An increasing salt concentration of the buffer causes fractional elution of protein. Streptavidin monomers, tetramers and aggregates can be identified by gel filtration with a sephacryl column. After sterile filtration, a UV/VIS spectrum of the solution is measured in order to determine its concentration.[8] The production of Traptavidin, Strep-Tactin is analogue. enhanced monomeric Avidin is isolated via IMAC.

A 50 ml preculture with E.coli BL 21/R carrying the pSUMO plasmid is poured into a shaking flask with 2 L LB medium. After the bacterial suspension reaches an optical density of 0.5 the production of PAS-Lysine is induced by adding IPTG (1 mM). The cells are harvested (5000 rpm, 30 minutes) after five hours and resuspended in 20 mM Tris/HCl buffer with 500 mM salt, pH 8. The cells are homogenized by French press or PANDA and centrifuged at 11500 rpm for 30 minutes. SUMO PAS-Lysine is very good soluble and therefore occurs in the supernatant, the pellet is discarded. SUMO PAS-Lysine has the property to remain native even at high temperatures, where most protein denaturate. Heating the solution up to 70 °C for 20 minutes and centrifugation afterwards removes nearly all other proteins. The solution is dialysed against IMAC buffer (50 mM sodium dihydrogen phosphate and 500 mM salt, ph 8) and injected on a chromatography column packed with nickel. After washing away impurities, the addition of imidazole results in elution of the SUMO PAS-Lysine. The SUMO domain has no further use and is cleaved off by the SUMO-protease ULP ( ). Another IMAC chromatography separates the PAS-Lysine from SUMO domain, which binds specifically to the column. PAS Lysine can be identified in the flow through via UV absorption. Because PAS-Lysine does not contain aromatic residues, its absorption at 280 nm is very low, while the absorption at 225 nm (amid bondage) is remarkably high. The proper fractions are pooled and the solution is dialysed against a physiologically buffer like 20 mM Tris/HCl with 500 mM salt, pH 8. The linker molecule can now be biotinylated.

Frozen HEK 293T cells, having been stored in liquid nitrogen, were quickly thawed in a 37°C water bath. Cells were then transferred into a tube containing pre-warmed Dulbecco’s Modified Eagle Medium medium (DMEM, including 10% fetal calf serum, 100 U/ml penicillin and 100 μg/ml streptomycin). After having been spun down (300 g, 5 mins), the supernatant was discarded and the pellet resuspended in DMEM. The cell suspension was then transferred into culturing flasks and incubated at 37°C and 5% CO₂ until further use. When reaching confluency, medium was removed from culture flasks and cells were washed twice with PBS. Cells were then treated with trypsine solution (0.05% in 1x PBS) and incubated at 37°C and 5% CO2 for 5 mins. After transferring cells into a 50 ml tube and adding 45 ml of medium, cells were counted and passaged into new culture vessels as deemed suitable.

For the quantification of expression of either the receptor or of nanoluciferase-containing constructs (e.g. for the choice of signal peptides and quantification of hypoxia-dependent promoter activity), luciferase assays were conducted.

Therefore, 4x10⁴ cells were seeded into 6-well plates in 4 ml DMEM medium until reaching the desired confluency. For transfection, 100 μl OptiMEM were mixed with 3 μg DNA and 12 μl Turbofect, vortexed for 10 s and incubated at room temperature for 20 mins. After removing 1 ml of supernatant, the transfection mixture was added drop-wise and the plate was incubated at 37°C and 8.5% CO₂ overnight. The next day, medium was removed and DMEM medium (10% FCS, Pen/Strep) was added.

For the luciferase assay, 50 μl of carefully removed medium were mixed with 50 μl luciferase assay buffer/sustrate mix from the NanoGlo Luciferase Assay Kit, and incubated for 10 mins at RT. Measurements were performed at 460 nm using a platereader.

For the analysis of the gene expression of the different receptors on mRNA level RT-qPCR was performed.

Thus 1x10⁶ and 1x10⁵ cells were collected and spun down. The medium was discarded. QIAzol was added to the cell pellet and mRNA extraction was performed according to manufacturer's protocol (miRNeasy micro kit, QIAGEN). Afterwards mRNA concentration was measured by nanodrop. In addition the total mRNA was analysed for purity and integrity with an Bioanalyzer (Agilent Technologies). The measurement with a RNA Nano Chip was performed according to manufacturers protocol (Agilent technologies).^[1]. To prepare the mRNA for quantitative analysis 750 ng of each sample mRNA were used for reverse transcription (RT).

The mastermix for the RT reaction was mixed as following:

Three reverse transcriptase negative (Neg. RT) samples as well as two controles without template mRNA were added as negative controls. The RT was performed according to manufacturer's protocol (????).

The generated cDNA was then used for the quantitative PCR. The analysis was conducted on a Biorad CFX 1000 with 348 block using the SsoFast EvaGreen PCR mix.

The ΔΔC_P method ^[2] is a method for relative quantification of expression level based on the comparison of C_P values for the specific mRNA of cells with the gene of interest (GOI) to those without the GOI in combination with the C_P values of a house keeping gene.

To explain the method you can take a look at the sample calculation below:

For confirmation of the molecular weight of proteins, electron spray ionisation-quadrupole time of flight was used. Protein masses were determined as a result from the mass/charge ratio (m/z). Herefore, 50-100 μl of a 0.1 mg/ml protein solution were dialyzed with 10 mM ammonium acetate (pH 6.6) overnight. For measurements, a mixture of 140 μl 10 mM ammonium acetate (pH 6.6), 40 μ acetonitrile, 20 μl of the dialized protein solution and 1 μl formic acid ( was injected.

For the analysis of protein binding affinities and kinetics, surface plasmon resonance spectroscopy was used.

Fluorescence titration is a method that utilizes the change of intrinsic protein fluorescence upon ligand binding (as mainly mediated by aromatic amino acid side chains) in order to quantify binding properties. This way, the binding affinity (as characterized by the K_D value) can be determined.

For the measurement, 2 ml of continuously stirred protein solution (1 μM) were titrated by the continuous addition of 100 μM D-biotin solution. For the measurements, temperatures of 20°C, an excitation wavelength of 295 nm and emission wavelengths of 350 nm were used (slid width of 5 mm, respectively) and the signal integrated over 5 s. The titrant was hereby added in 2 μl steps until a final titrant concentration of 2 μM.

For the analysis of protein folding states, circular dichroism spectroscopy was used, as it allows drawing conclusions about the formation of protein secondary structures.

For that purpose, three CD spectra were recorded, for each of which a 10 μM protein concentration according to the respective monomer and a cuvette with a 1 mm thickness was used. First, a UV-CD spectrum at 20°C was recorded with a start wavelength of 250 nm and an end wavelength 190 nm. Second a denaturation spectrum and third, a renaturation spectrum was recorded, both of which were recorded at 213 nm between 20 and 95 °C. As an exception, enhanced monomeric avidin was measured at 203 nm.