Inducible, Cell Type-Specific Expression in Arabidopsis thaliana Through LhGR-Mediated Trans-Activation

Podsumowanie

Here, we describe the generation and application of a set of transgenic Arabidopsis thaliana lines enabling inducible, tissue-specific expression in the three main meristems, the shoot apical meristem, the root apical meristem, and the cambium.

Streszczenie

Inducible, tissue-specific expression is an important and powerful tool to study the spatio-temporal dynamics of genetic perturbation. Combining the flexible and efficient GreenGate cloning system with the proven and benchmarked LhGR system (here termed GR-LhG4) for the inducible expression, we have generated a set of transgenic Arabidopsis lines that can drive the expression of an effector cassette in a range of specific cell types in the three main plant meristems. To this end, we chose the previously developed GR-LhG4 system based on a chimeric transcription factor and a cognate pOp-type promoter ensuring tight control over a wide range of expression levels. In addition, to visualize the expression domain where the synthetic transcription factor is active, an ER-localized mTurquoise2 fluorescent reporter under control of the pOp4 or pOp6 promoter is encoded in driver lines. Here, we describe the steps necessary to generate a driver or effector line and demonstrate how cell type specific expression can be induced and followed in the shoot apical meristem, the root apical meristem and the cambium of Arabidopsis. By using several or all driver lines, the context specific effect of expressing one or multiple factors (effectors) under control of the synthetic pOp promoter can be assessed rapidly, for example in F1 plants of a cross between one effector and multiple driver lines. This approach is exemplified by the ectopic expression of VND7, a NAC transcription factor capable of inducing ectopic secondary cell wall deposition in a cell autonomous manner.

Wprowadzenie

A major limitation in biology in the postgenomic era is to decipher the context specific role of a given factor or genetic perturbation. Constitutive genetic perturbations such as loss-of-function and gain-of-function approaches often only allow end-point analysis of life-long adaptation processes, obfuscating the distinction between primary and secondary effects. In addition, context specific functions can be masked or diluted by large scale effects in distant tissues or during other phases of development. Moreover, in extreme cases, lethality can preclude any mechanistic insight. Ideally, to circumvent these issues, one could analyze the effect of acute genetic perturbation within a specific context such as a specific cell type in a time-resolved manner. To achieve this, genetic tools for inducible, cell type-specific expression are required¹. To provide a resource for the rapid assessment of the spatiotemporal dynamics of a response to a given effector, we have combined the ease of cloning provided by the GreenGate system² with the proven efficacy of the GR-LhG4 system^3,4,5,6. We have generated a set of lines expressing the chimeric transcription factor LhG4 fused to the ligand binding domain of the rat corticoid receptor (GR)⁷ under the control of well-characterized cell type specific promoters⁸. In resting conditions, the transcription factor remains outside of the nucleus, as the GR domain is bound by the cytosolic HSP90. With the addition of synthetic ligand dexamethasone (Dex), nuclear translocation is induced and LhG4 will mediate transcription of expression cassettes under control of a cognate synthetic pOp-type promoter, such as an mTurquoise2 reporter included in the driver lines to visualize the expression domain after induction.  Thus, the driver lines technically also contain an effector cassette. The crossing of a set of driver lines with a line carrying an effector cassette with, for example, a gene of interest under control of the same pOp-type promoter thus allows the rapid assessment of the acute or long-term consequences of effector expression in a wide range of cell types.

Here, we provide a protocol describing the procedures necessary to generate the driver and effector lines and demonstrate how cell type specific expression can be induced and followed in the shoot apical meristem, the root apical meristem and the cambium of Arabidopsis. To illustrate the prowess and specificity of this approach, we utilize the well-known transcription factor VND7 which is capable of driving xylem-like secondary cell wall thickenings ectopically⁹. Treating F1 from a cross between the pSCR^10,11 driver line and the pOp6:VND7 effector line leads to the formation of ectopic xylem-like cells in the starch sheath cells of the Arabidopsis stem.

To facilitate the generation of large DNA assemblies required for constructing driver and effector expression plasmids, we used the fast and efficient GreenGate cloning method². GreenGate cloning is based on type II S restriction enzymes such as Eco31I or its isoschizomer BsaI². These enzymes cut downstream of their asymmetric recognition sites producing overhangs with varying base composition. By incorporating Eco31I/BsaI restriction sites in oligonucleotides and allocating specific overhang sequences to DNA elements, modular cloning is achieved, facilitating the generation of large assemblies. In the GreenGate framework, DNA modules fall into categories A-F based on overhang sequence that serve as adapters and are assembled in that order. Therefore, the primers designed to amplify your desired product should be in accordance with the selected module² (Figure 1A). If there is an internal Eco31I/BsaI site and the sequence is not compatible with the GreenGate entry and destination modules, you can proceed without mutagenizing, but with lower efficiency. Alternatively, use site-directed mutagenesis to remove Eco31I/BsaI restriction sites taking care not to change amino acids in gene products.

Protokół

Vectors and modules can be obtained from the non-profit repository, Addgene (https://www.addgene.org).

1. Cloning using GreenGate

1. Design primers using the overhangs listed in Table 1, replacing ‘NNNN’ with module type-specific adapter sequences listed below: Forward: 5´AACA GGTCTC A NNNN (n) CA^* + specific sequence 3´, Reverse: 5´AACA GGTCTC A NNNN (n) + reverse complement of specific sequence 3´. Add the underlined bases to ensure maintenance of the reading frame.
   Module overhangs:
   ​NOTE: In the default GreenGate framework, six modules, A-F, are assembled with a plant transformation vector backbone into one expression plasmid (Figure 1C). Typically, the A module will harbor promoter sequences, a B-module an N-terminal tag or “dummy” sequence⁶, a C-module a CDS, a D-module a C-terminal tag or dummy, an E-module a terminator, and an F-module a resistance cassette for selection of transgenic plants. Adapter for coupling with other preassembled units are available for use instead of the F module².
2. PCR amplification
   1. Amplify the sequence of interest with the designed primers by polymerase chain reaction (PCR) according to standard protocols.
   2. Separate the PCR product on an agarose gel. Excise and column purify the correct fragment using a commercial kit (see Table of Materials) as per the manufacturer’s instructions.
3. Entry module creation
   1. Separately digest the module vector and the PCR fragment (step 1.2.) (Figure 1 A, B) with Eco31I/BsaI using 100-500 ng of DNA (Vector or Fragment), 3 µL 10x digestion buffer, and 5-10 U Eco31I in a tube and bring the volume to 30 µL with ddH₂O.
   2. Mix gently by pipetting up and down and spin down briefly at 1,000 x g. Incubate at 37 °C on a heat block for 15 min (or following the time recommendation of the purchased restriction enzyme).
   3. After the digestion, column purify each sample using a commercial kit (see Table of Materials) and quantify the obtained DNA by determining the optical density at 260 nm (OD₂₆₀) using a spectrophotometer.
   4. Mix the 30 – 100 ng digested insert and the 10 – 50 ng digested vector by pipetting up and down several times and incubate with 1 µL T4 Ligase (5 U/µL, and 3 µL 10 x T4 ligation buffer in a total volume of 30 µL at room temperature for 1 h (following the recommendation of the T4 ligase supplier) (see Table of Materials).
      NOTE: Calculate the desired molar ratio entry module:destination vector (e.g., 3:1) for the ligation depending on the concentration and length of the entry module inserts.
   5. To increase the efficiency of transformation, heat inactivate the T4 ligase by Incubating the reaction at 65 °C for 20 min.
   6. Use the ligation product to transform competent E. coli cells according to the standard lab protocols and spread the bacteria on agar plates supplemented with ampicillin (100 µg/mL)
   7. Incubate the plate with bacteria at 37 °C for overnight.
   8. Screen for colonies with the desired entry module by colony PCR using the primers 86A1 (5′-GTTGTGTGGAATTGTGAGC-3′) and 86A2 (5′-GTTTTCCCAGTCACGACG-3′) and standard PCR conditions.
      NOTE: This primer combination is valid for all entry modules as the primers bind to the entry vector backbone.
   9. Select single colonies for the plasmid isolation. Use 2 mL LB liquid culture supplemented with ampicillin (100 µg/mL) and incubate overnight in a 37 °C shaker.
   10. Isolate plasmids from the overnight liquid culture with a Mini-Prep Kit or the desired extraction protocol (see Table of Materials).
   11. To identify plasmids with the correct insert, perform restriction enzyme analysis, for example by selecting two enzymes that cut uniquely in your insert by mixing 200 ng of plasmid, 2 µL 10 x digestion buffer, 5-10 U of selected restriction enzymes and ddH₂O to 20 µL.
   12. Sequence the selected plasmids using the primers 86A1 and 86A2 (see step 1.3.9.).
4. Destination module creation:
   NOTE: For the destination plasmid use the desired destination module pGGZ001, pGGZ002 or pGGZ003² (Figure 1C).
   1. In a tube add and mix 50 – 150 ng empty destination vector (pGGZ003, for example), 50-300 ng of each filled entry module, 2 µL 10 x digestion buffer buffer, 1.5 µL 10 mM ATP, 1 µL T4 Ligase (30 U/µL), 5-10 U µL Eco31I and dH₂O to a total volume of 20 µl.
      NOTE: Calculate the desired molar ratio entry module:destination vector (e.g. 3:1) for the ligation depending on the concentration and length of the entry module inserts.
   2. Mix and perform the GreenGate reaction² using a PCR thermocycler alternating 30 times between 37 °C for 5 min and 16 °C for 2 min, followed by single steps of 5 min at 50 °C and 5 min at 80 °C.
   3. To increase the efficiency, add 1 µL T4 Ligase (30 U/µL) and 1.5 µL 10 mM ATP to the reaction and incubate for 1 h at room temperature, followed by heat-inactivation of T4 DNA Ligase at 65 °C for 20 min.
   4. Use the ligation reaction to transform competent E. coli and spread the bacteria on agar plates supplemented with the appropriate selective agent spectinomycin (50 µg/mL).
   5. Incubate the transformed E. coli on the plate at 37 °C for overnight.
   6. To confirm transformation, re-streak each of the selected single colonies on spectinomycin (50 µg/mL) and ampicillin (100 µg/mL) containing plates, respectively. Use only colonies that grow on spectinomycin but not on ampicillin plates.
   7. Incubate the E. coli colonies overnight at 37 °C.
   8. Select single colonies for plasmid isolation. Use 2 mL LB liquid culture supplemented with spectinomycin (50 µg/mL) and incubate overnight at a 37 °C shaker.
   9. Isolate the corresponding plasmids with a Mini-Prep Kit (see Table of Materials).
   10. Check by restriction enzyme analysis (see 1.3.12.) and sequence selected positive constructs using primers 88C3 (5′-ACCTCTCGGGCTTCTGG-3′), 88C4 (5′-CCTTTTTACGGTTCCTG-3′). If the insert cannot be fully sequenced with these primers, design internal primers for sequencing.
       NOTE: To identify clones with the correct number of pOp repeat sequences (see Discussion), the primers pOp6 (pOp6_F, 5′-TGCATATGTCGAGCTCAAGAA-3′; and pOp6_R, 5′-CTTATATAGAGGAAGGGTCTT-3′) that bind in the short flanking sequences can be used for PCR amplification and subsequent gel electrophoresis to discriminate by size.
5. Intermediate supermodule creation
   1. To combine two independent sets of entry modules, as required for generating the GR-LhG4 driver lines with integrated reporter-effector cassette, first build two intermediate plasmids, called supermodules², before assembling the final expression plasmid in pGGZ001 or pGGZ003.
   2. Be sure to add F-H adaptor at the end of the first supermodule and H-A adaptor at the beginning of the second supermodule (those serve as connections between two constructs) as described².
      NOTE: Only the pGGN000 intermediate module carries the resistance cassette. To generate the expression plasmid, perform the GreenGate reaction with the destination vector and the pGGN000 and pGGM000 intermediate supermodules. Alternatively, mix destination vector, pGGN000 intermediate supermodule, and the remaining single modules to perform the GreenGate reaction². The latter method is less efficient than the former but can be faster.
   3. To create a pGGM000/pGGN000 supermodule, mix 1.5 µL (100-300 ng/µL) of each of the entry modules with 1 µL (30 ng/µL) empty intermediate vector (pGGM000 or pGGN000), 2 µL 10 x digestion buffer, 1.5 µL 10 mM ATP, 1 µL T4 Ligase (30 U/µL), and 5-10 U Eco31I in a total volume of 20 µL.
      NOTE: Calculate the desired molar ratio entry module:destination vector (e.g., 3:1) for the ligation depending on the concentration and length of the entry module inserts
   4. Mix and perform the GreenGate reaction as in step 1.4.2
   5. To increase efficiency, add 1 µL T4 Ligase and 1.5 µL ATP (10 mM), and incubate for 1 h at room temperature, followed by heat-inactivation at 65 °C for 20 min.
   6. Use 10 µL of the ligation reaction to transform competent E. coli and streak on plates containing kanamycin (50 µg/mL).
   7. Perform overnight incubation of the transformed E. coli on the plate at 37 °C.
   8. Re-streak each of the selected single colonies on kanamycin (50 µg/mL) and ampicillin (100 µg/mL) containing plates, respectively.
   9. Perform overnight incubation of the E. coli colonies on the plate at 37 °C.
   10. Select single colonies that grow only on kanamycin but not on ampicillin for plasmid isolation. Use 2 mL LB liquid culture supplemented with kanamycin (50 µg/mL) and incubate overnight in a 37 °C shaker.
   11. Isolate the corresponding plasmids using a mini-prep kit (see Table of Materials).
   12. Check the plasmids by restriction enzyme analysis (see 1.3.12.)and confirm by sequencing using primers 87E2 (5´-AGGCATCAAACTAAGCAGAAG-3´) and 87E3 (5´-CGTTTCCCGTTGAATATGGC-3´) annealing to the pGGM000/pGGN000 backbone. If the insert cannot be fully sequenced with these primers, design internal primers for sequencing.
       NOTE: If cloning into the pGGM000 or pGGN000 vectors is unsuccessful, one possible solution is to digest the pGGM000 or pGGN000 with Eco31I, run on a gel and purify from the gel the pGGM000 or pGGN000 backbone (approximately 2000 bp) fragment without the ccdB cassette (approximately 1400 bp). Then proceed normally with the ligation reaction.
6. Transform an A. tumefaciens pSOUP⁺ strain (e.g. ASE), as the pSa origin of replication (ori A. tum.) in the destination vectors require the presence of the helper plasmid pSOUP¹². Streak out bacteria on LB plates containing chloramphenicol (34 µg/mL), kanamycin (50 µg/mL), spectinomycin (50 µg/mL) and tetracycline (12.5 µg/mL). Incubate the transformed A. tumefaciens on the plate in a 28 °C incubator for two to three days.

2. Generation of Arabidopsis transgenic plants

1. Transformation of Arabidopsis thaliana.
   NOTE: Transform A. thaliana plants according to Zhang et al., 2006¹³.
2. Selection of transgenic lines.
   1. To select the transformed plants, use the selection scheme used at GABI-Kat¹⁴ for resistance to sulfadiazine¹⁵.
   2. To select stable lines with a possible single integration event, choose those in generation T2, that show the 3:1 segregation ratio in the resistance marker. Propagate these lines to T3 generation and select the plants homozygous for the resistance gene. Alternatively, perform a Southern Blot analysis or a standard quantitative real-time PCR (SA-qPCR)¹⁶ to select single insertion lines.

3. Induction of trans-activation in Arabidopsis driver lines

1. Root
   1. To test reporter expression in A. thaliana driver lines generated through steps 1 and 2, sterilize seeds as described below.
      1. Add 0.5-1.0 mL of 70 % Ethanol + 0.01 % non-ionic detergent to approximately 100 seeds (20 mg) in a 1.5 ml reaction tube and invert the tube a few times. Spin down at 1000 x g for 15 s and aspirate the supernatant.
      2. Add 0.5-1.0 mL of absolute ethanol. Invert the tube several times, spin down for 1,000 x g for 15 s and discard the supernatant.
      3. Add 0.5-1.0 mL of absolute ethanol and invert the tube t a few times, then spin down at 1,000 x g for 15 s and discard the supernatant.
      4. Allow seeds to dry inside the hood. If seeds are going to be stratified in tubes continue with step 3.1.1.6.
      5. Add 0.5-1.0 mL of sterile water and invert the tube a few times. Spin down at 1,000 x g for 15 s and discard the supernatant.
      6. Add 0.5-1.0 mL of sterile water and invert the tube several times. Spin down at 1,000 x g for 15 s and discard the supernatant.
      7. Add 0.5-1.0 mL of sterile water.
   2. Prepare half-strength Murashige and Skoog medium, pH 5.8 and add 0.9% plant agar and 1% sucrose. After autoclaving add Dexamethasone (Dex), dissolved in DMSO, to a final concentration of 10 - 30 µM to induction plates and an equal amount of DMSO to control plates, respectively.
   3. Put seeds for root imaging on plates and stratify them for 48 h in darkness and cold (4 °C).
   4. Put plates in a vertical position in a plant incubator (long day (16/8 h), 22 °C, humidity, 65 %) and grow them for five days.
   5. Five days after germination (dag), image the seedlings using confocal laser scanning microscopy.
2. Stem
   1. Sterilize seeds as described in 2.1.1. and put seeds on ½ MS, 0.9% plant agar and 1 % sucrose plates. Stratify for 48 h in darkness and cold (4 °C).
   2. Six to seven days after germination, transfer the seedlings to soil, each plant in a single pot (long day (16/8 h), 22 °C, humidity, 65%).
   3. Induce trans-activation in stems by watering with Dex or mock solution, or by dipping the plants in Dex or mock solutions, respectively.
   4. For watering, use a 25 µM Dex solution in water prepared from a stock of 25 mM Dex dissolved in ethanol. Water every 2-3 days until the desired time of induction.
   5. For dipping, prepare a 1 L beaker, 750 mL of water containing 0.02% silwet L-77 with 25 µM of Dex or equivalent amount of DMSO for the Dex and mock treatment, respectively. Dip single plants for 30 s in the induction or in the mock solution. Repeat every 2-3 days until the desired time of imaging.
      NOTE: Following the dipping, the plants should be maintained in high humidity for one hour.
3. Shoot Apical Meristem (SAM)
   1. Sterilize seeds as described in 2.1.1. Prepare plates with ½ MS, 0.9 % plant agar and 1 % sucrose medium and put seeds on plates. Store the plates for two days in darkness and cold for stratification.
   2. Put plates in a vertical position in a plant incubator. Six to seven days after germination, transfer the seedlings to the soil, each plant in a single pot (long day (16/8 h), 22 °C, humidity, 65 %).
   3. When the stem is around 1 cm long (25-30 dag), spray the inflorescence SAM with 10-50 µM Dex in H₂0 wearing a face mask. For induction and imaging at later stages of development, induce SAMs of longer stems or side shoots.
      NOTE: SAMs can also be induced by paintbrushing the Dex solution to prevent spray droplets. Do use a mask when Dex is applied by spraying.
   4. 24-48 h after induction, dissect the SAMs and proceed to imaging (see 4.3).
      NOTE: Only un-induced plants were used for propagation to reduce the probability of gene silencing. Plants in T2/T3 were used for imaging.

4. Imaging of reporter expression in Arabidopsis driver lines.

1. Root
   1. Transfer seedlings from plate to a 10 µg/mL propidium iodide (PI) solution and counter-stain them for 5 min.
   2. Place the roots into a microscope imaging chamber (1-well tissue culture chamber on cover glass II, see Table of Materials) and image them using a confocal laser scanning microscope with a 63x water immersion objective (see Table of Materials).
   3. To visualize PI fluorescence, use an excitation wavelength of 488 nm and collect emission between 590 and 660 nm. For mTurquoise2 fluorescence use 458 nm excitation and collect emission between 460 and 615 nm.
2. Stem
   1. Perform horizontal hand cut sections of plant stems with a razor blade, excising a segment of approximately 3 cm. Fix the stem with the finger on the opposite side of the desired section to cut. Perform several fine cuts sequentially but note that only sections from a similar position in the stem should be compared.
   2. After each cut, immerse the razorblade in a petri dish containing tap water and collect the stem sections. Stain sections at this point or directly mount on microscope slides.
   3. For staining, prepare a 1 mL of 250 µg/mL of PI solution of water in a small petri dish (see Table of Materials). Immerse the sections for 5 min and rinse them in water. Transfer them to microscope slides with fine forceps or a fine paint brush. Take care to not squeeze the samples with the coverslip.
   4. Image samples using a confocal laser scanning microscope with a 25x dipping water immersion lens (see Table of Materials). Use 561 nm laser light to excite PI fluorescence and collect from 570 to 620 nm. Use 405 nm to excite the mTurquoise2 fluorophore effector encoded by the driver line constructs and collect emission from 425 to 475 nm.
3. Shoot Apical Meristem
   1. Cut the stem 2 cm below the shoot tip with forceps. Hold the stem in one hand and use fine forceps to remove the flower buds and large primordia. To remove young primordia, fix the SAM in an upright position into a petri dish containing 3 % agarose. Use a binocular and forceps to remove young primordia close to the SAM. Alternatively, use an injection cannula (see Table of Materials) to cut off these primordia.
   2. Stain the dissected SAM in a 250 µg/mL PI solution for 5-10 min. Perform staining either directly by pipetting a few drops of staining solution on top of the prepared SAM or transfer the sample to a tube filled with staining solution. Keep the SAM fully submerged during the staining procedure.
   3. Place the stained SAM into a small petri dish (see Table of Materials) with 3 % agarose medium and cover the SAM with ddH₂O.
   4. Image dissected SAMs using a confocal laser scanning microscope equipped with a 25 x dipping water immersion lens (see Table of Materials).
   5. Use 561 nm laser light to excite PI fluorescence and collect from 570 to 620 nm. Use 405 nm to excite the mTurquoise2 fluorophore and collect emission from 425 to 475 nm.
      Record image stacks spanning 50 µm in z-direction with a step size of 0.5 µm.
      NOTE: SAM imaging as described here requires an upright confocal laser scanning microscope and a lens (here, a water dipping lens) with long working distance.

Wyniki

Generation of driver and effector lines through GreenGate cloning

The GreenGate cloning system is based on GoldenGate cloning and use the type IIS restriction endonuclease BsaI or its isoschizomer Eco31I. As the enzyme produces overhangs distant from its asymmetric recognition site, the base composition of the overhangs can be freely chosen, which is the basis form the modularity of the system. Each PCR-generated element, for example, a promoter sequence, CDS...

Dyskusje

Here, we describe the steps necessary to generate and apply a versatile and comprehensive toolkit for inducible, cell type specific trans-activation. Crossing lines carrying effector cassettes under control of the pOp promoter with driver lines allows studying the mis-expression effects in the F1 generation, enabling the rapid assessment of genetic perturbation in a wide range of cell types. Alternatively, effector constructs can be used to transform driver lines or, by adapting the cloning strategy, dr...

Materiały

Name	Company	Catalog Number	Comments
Ampicillin	Carl Roth GmbH + Co. KG	K029.1
ATP	Sigma-Aldrich	A9187
Chloramphenicol	Sigma-Aldrich	C1919
Column purification	Qiagen	QIAquick PCR Purification Kit (250)
Culture chamber for imaging	Sarstedt AG & Co. KG	1-well tissue culture chamber, on cover glass II
Dexamethasone	Sigma-Aldrich	D4903
DMSO	Fisher Scientific, UK	D139-1
Eco31I	Thermo Fisher Scientific	FD0294
injection cannula (0.30 x 12 mm, 30 G x 1/2)	Sterican, Braun
Kanamycin	Carl Roth GmbH + Co. KG	T832.2
Leica TCS SP5 CLSM, HCX PL APO lambda blue 63x water immersion objectiv	Leica, Wetzlar, Germany
MS medium	Duchefa, Haarlem, Netherlands	M0221.0050
Nikon A1 CLSM, Apo LWD 25x  1.1 NA water immersion objective	Nikon, Minato, Tokyo, Japan
Petri dish 35/10 mm	Greiner Bio-One GmbH, Germany	627102
Petri dish 60/150 mm	Greiner Bio-One GmbH, Germany	628102
Petri dish 120/120/17	Greiner Bio-One GmbH, Germany	688102
Plant agar	Duchefa, Haarlem, Netherlands	P1001
Plasmid extraction	Qiagen	QIAprep Spin Miniprep Kit
Propidium iodide (PI)	Sigma-Aldrich	P4170
Razorblade	Classic, Wilkinson Sword GmbH	7005115E
Reaction tubes	Sarstedt AG & Co. KG	72.690.001
Silwet L-77	Kurt Obermeier GmbH & Co. KG, Bad Berleburg, Germany
Spectinomycin	AppliChem GmbH	3834.001
Spectrophotometer	Thermo Fisher Scientific	NanoDrop 2000c
Sucrose	Carl Roth GmbH + Co. KG	4621.1
Sulfadiazine	Sigma-Aldrich	S6387
Tetracycline	AppliChem GmbH	2228.0025
T4 Ligase 5 U/µl	Thermo Fisher Scientific	EL0011
T4 Ligase 30 U/µl	Thermo Fisher Scientific	EL0013