Team:Hawaii/Initial Synth. Oligo Assembly

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Contents

Protocol

Hybridization of Parts

  1. Mix:
    3 μl 100 µM sense oligo
    3 μl 100 µM anti-sense oligo
    3 μl 10 x PNK (polynucleotide kinase) buffer
    2 μl 10mM ATP
    2 μl T4 polynucleotide kinase (PNK)
    17 μl distilled water
    Total volume = 30 μl
  2. Incubate at 37C for 1.5 hours.
  3. Add 4 μl 0.5 M NaCl.
  4. Place in boiling water bath for 2 min., then remove water bath from the heat source and allow the reaction (still in the water bath) to cool to room temperature (approx. 30 minutes)
Reference: Pam Silver Lab. [http://openwetware.org/wiki/Silver:_Oligonucleotide_Inserts| Oligonucleotide Inserts.]

DNA Ligation

  1. Combine 4 ul of construct one with 4 ul of construct 2.
  2. Add 1 ul of nanopure H20.
  3. Add 10 ul of 2x quick ligation reaction Buffer. In order to avoid shearing the DNA, mix by resuspending very slowly.
  4. Add 1 ul of Quick T4 DNA ligase and mix thoroughly by resuspending very slowly.
  5. Incubate at room temperature for 5 minutes.
  6. Cool on ice then transform, or store at -20oC
Reference: Quick Ligation Kit from NEB.

Restriction Enzyme Digest

  • May not be necessary
  1. Add REs in appropriate amounts to appropriate buffer (check if enzymes are compatible).
  2. Incubate at least 1 hour at recommended temperature (usually 37C).
  3. Stop reaction by adding 5 μl 10X loading buffer or by incubating 10 min. at 65C.

Notes:

  • <10% of digest should be RE
  • REs are stored in glycerol. <5% glycerol should be present in digest. Therefore, a minimum 10-fold dilution is necessary so the enzymes don't act funky.
  • It's always a good idea to gently shake and spin down RE and RE buffer prior to use.
Reference: Short Protocols in Molecular Biology. Vol. 1. 5th edition. 3-3 to 3-4.

Results

First attempt

Nice bands observed for annealed oligos. Bands appear to be the correct size (<100bp) but we can't tell if anneal worked (EtBr doesn't tell us if these are ssDNA or dsDNA bands). Smear is probably from loading way too much DNA (see discussion). Possible faint band for pnir ligation. No bands for slr2016 and pilA ligation, probably because way too much DNA was added for the ligation reaction.

Second attempt

Did a ligation using 1 μl of a 10-6 dilution of each annealed product. Ligated at both room temperature and at 40C (recommended by Frank, etal). Nothing was visible on the EtBr stained 4% agarose gel because not enough DNA was present.

Third attempt

Did a ligation using 10-2 dilutions of annealed product (ligated at room temperature and at 40C). Faint bands were visible for the annealed products (10-2 dilutions) but no bands were observed for the ligated products. Not enough DNA was present. Ran 10-1 dilutions of annealed product on SYBR Safe stained 2% agarose gel.

Fourth attempt

Took 10 μl ligation reaction from first attempt and restriction digested with XbaI and PstI (1 μl each) in NEBuffer 3 (1 μl). A ladder of bands were observed for the ligation product, indicating incomplete digestion.

Fifth attempt

Repeated ligation using full concentrations of annealed product. RE digested as in fourth attempt, with incubation for 2.5 hours. Loaded 20 μl of ligation into well with 2μl loading dye. Less loading dye was used so the bromophenol blue would not block out our band. Band(s) will not resolve on the gel if less than 20μl of the ligation is loaded.

Gel turned out funky (was it poured too late and the agarose already began solidifying?) Ladder did not run correctly but luckily, the pnirs did (we know their size). Also, from the fourth attempt gel, we knew the approximate location of ligation bands. Bands excised from the gel are circled in the figure below. For the slr2016 signal sequence ligation, no band was observed at the expected size. Very faint bands were observed above and below the expected ~80bp mark so both were excised and purified.

First assembly attempt. Ten microliters loaded into each well of an EtBr stained ~3% agarose gel ran at 95V for 1 hr.
Third ligation attempt. Ten microliters loaded into each well of an EtBr stained 4% agarose gel ran at 95V for 28 min.
SYBR Safe stained 2% agarose gel ran at 95V for 30 min. Ten microliters of a 10-1 dilution of annealed product was loaded into each well.
Fourth attempt. Ten microliters of 10-1 dilution of annealed product or 1:1 ligation product was loaded into each well. Ran on EtBr stained 4% agarose gel at 95V for 30 min.
Fifth assembly attempt. Ten microliters of ladder, pnir1, and pnir2 loaded in wells. Twenty microliters of pnir1+2, slr1+2, and pilA1+2 loaded into wells. SYBR Safe stained 4% agarose gel ran at 95V for 50 min. Circled bands were extracted from the gel.




Plasmid prep and digestion of BBa_C0012 harboring vector

The plasmid prep was RE digested using XbaI and PstI per NBE's instructions. Distinct bands were observed the gel at 1.2kb and 2,4kb, corresponding to the lacI gene (BBa_C0012) and the vector. Comparing the intensity of the vector band to the ladder bands, it is estimated that there is ~40ng of vector.

Restriction digest of BBa_C0012. Twenty microliters of the digest were loaded onto an EtBr stained 0.8% agarose gel ran at 95V for 20 min.

Discussion

We need to dilute our annealed products before running them in a gel or attempting ligation. 20-125ng DNA (per lane) is good for running gels. One reaction using the NEB Quick Ligation Kit can ligate up to 180ng of DNA.

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