Team:Dalton School NY/Notebook

From 2012hs.igem.org

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(Testing of DNA prepared by several methods)
(Obtaining the remaining clones)
 
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In progress...
 
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==Testing of DNA prepared by several methods==
==Testing of DNA prepared by several methods==
-
Yeast genomic DNA is commonly prepared using a phenol/chloroform based method. Because both phenol and chloroform are toxic chemicals, we tested several methods for preparing yeast genomic DNA that do not use these chemicals. We compared a method that uses LiOAc to disrupt the yeast cell wall (BioTechniques 50:325-328, 2011) to methods that use the enzyme zymolyase to disrupt the cell wall (a Promega kit or a protocol from Jim Haber’s lab, “JH zym”). The Haber lab protocol produced the greatest yield of genomic DNA, but DNA made using the Promega kit was used in subsequent PCRs because it seemed to produce the most consistent results. 1µl, 2µl, or 5µl of genomic DNA was used in each PCR reaction with LIF1 promoter primers. Following these initial tests, 1µl of yeast genomic DNA was used for subsequent PCRs. The LiOAc method was the shortest and least expensive and we may switch to this method when future DNA preps are needed.
+
Yeast genomic DNA is commonly prepared using a phenol/chloroform based method. Because both phenol and chloroform are toxic chemicals, we tested several methods for preparing yeast genomic DNA that do not use these chemicals. We compared a method that uses lithium acetate (LiOAc) to disrupt the yeast cell wall ([http://www.biotechniques.com/multimedia/archive/00147/BTN_A_000113672_O_147315a.pdf BioTechniques 50:325-328, 2011]) to methods that use the enzyme zymolyase to disrupt the cell wall (a Promega kit or a [http://www.bio.brandeis.edu/haberlab/jehsite/pdfs/ZymoPrep.pdf protocol from Jim Haber’s lab], “JH zym”). For the Haber lab protocol, we did not include beta mercaptoethanol (also toxic) in the zymolyase solution, realizing that without this the zymolyase step might take longer. We used the procedure in the Haber lab protocol to check the completion of the zymolyase digestion for the Promega protocol and the Haber lab protocol. DNA from all protocols was treated with RNase A. The Haber lab protocol produced the greatest yield of genomic DNA, but DNA made using the Promega kit was used in subsequent PCRs because it seemed to produce the most consistent results. 1µl, 2µl, or 5µl of genomic DNA was used in each PCR reaction with LIF1 promoter primers. The exception was that the DNA prepared using the Haber lab protocol was diluted 1:10 because it was about 10X more concentrated than the DNA prepared using the other methods. Following these initial tests, 1µl of yeast genomic DNA was used for subsequent PCRs. The LiOAc method was the shortest and least expensive and we may switch to this method when future DNA preps for PCR are needed. It should be noted that in retrospect, the PCR reactions below were too robust to fairly compare the DNA preps. DNA would need to be diluted and/or the cycles would need to be shortened to come close to having PCR reactions in the linear range. However, we learned from this that we had successfully prepared genomic DNA, so we moved forward.
 +
 +
For PCR, we used:
 +
 +
:Yeast Genomic DNA: 1µl or 2µl or 5µl
 +
 +
:2X OneTaq Mix (NEB): 25µl
 +
 +
:5µM Forward primer: 2.5µl
 +
 +
:5µM Reverse primer: 2.5µl
 +
 +
:H2O: 19µl or 18µl or 15µl
 +
 +
 +
 +
'''Cycling conditions'''
 +
 +
:1 cycle of:
 +
 +
::94°C 5 min
 +
 +
:15 cycles of:
 +
 +
::94°C 30 sec
 +
 +
::50°C 30 sec
 +
 +
::68°C 45 sec
 +
 +
:30 cycles of:
 +
 +
::94°C 30 sec
 +
 +
::55°C 30 sec
 +
 +
::68°C 45 sec
 +
 +
:1 cycle of:
 +
 +
::68°C 5 min
 +
 +
2% agarose gels in 1X Sodium Borate buffer: [http://www.biotechniques.com/multimedia/archive/00036/BTN_A_04362BM02_O_36180a.pdf BioTechniques 36:214-216 (February 2004)]
 +
 +
"LiOAc (liq)" = Lithium acetate, prepped from yeast in liquid culture
 +
 +
"LiOAc (col)" = Lithium acetate, prepped from a yeast colony
 +
 +
"JH zym" = Prepped with Haber lab zymolyase protocol
 +
 +
"Promega" = Prepped with Promega Wizard Genomic DNA kit
[[Image:Dalton_Fig7.jpg]]
[[Image:Dalton_Fig7.jpg]]
Line 10: Line 58:
==PCR of promoters and fluorescent protein coding sequences==
==PCR of promoters and fluorescent protein coding sequences==
-
We did an isolation of genomic DNA from yeast using the Promega Wizard Genomic DNA Purification Kit- cat# A1120. We substituted 20T zymolyase (Seikagaku) for lyticase.
+
We did an isolation of genomic DNA from yeast using the Promega Wizard Genomic DNA Purification Kit- cat# A1120. We substituted 20T zymolyase (Seikagaku) for lyticase and monitored the zymolyase digestion for completion.
 +
 
 +
PCR primers were designed by students and supplied by IDT.
For PCR, we used:
For PCR, we used:
-
Yeast Genomic DNA: 1µl
+
:Yeast Genomic DNA: 1µl   OR  1µl of 5ng/µl fluorescent protein plasmid
 +
 
 +
:2X OneTaq Mix (NEB): 25µl
 +
 
 +
:5µM Forward primer: 2.5µl
 +
 
 +
:5µM Reverse primer: 2.5µl
 +
 
 +
:H2O: 19µl
 +
 
 +
 
 +
 
 +
'''Cycling conditions'''
 +
 
 +
:1 cycle of:
 +
 
 +
::94°C 5 min
 +
 
 +
:15 cycles of:
 +
 
 +
::94°C 30 sec
 +
 
 +
::50°C 30 sec
 +
 
 +
::68°C 45 sec
 +
 
 +
:30 cycles of:
 +
 
 +
::94°C 30 sec
-
2X OneTaq Mix (NEB): 25µl
+
::55°C 30 sec
-
5µM Forward primer: 2.5µl
+
::68°C 45 sec
-
5µM Reverse primer: 2.5µl
+
:1 cycle of:
-
H2O: 19µl
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::68°C 5 min
The ladder on all gels is the 2-log ladder (NEB).
The ladder on all gels is the 2-log ladder (NEB).
-
2% agarose gels in 1X Sodium Borate buffer: BioTechniques 36:214-216 (February 2004)
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2% agarose gels in 1X Sodium Borate buffer: [http://www.biotechniques.com/multimedia/archive/00036/BTN_A_04362BM02_O_36180a.pdf BioTechniques 36:214-216 (February 2004)]
[[Image:Dalton_Fig6.jpg]]
[[Image:Dalton_Fig6.jpg]]
Line 34: Line 112:
There may be more nonspecific bands in these PCR reactions than is typical either because there was a considerable delay waiting for all students to be ready to add their tubes to the PCR machine or because we had an issue where the program was initially incorrect and we needed to restart the PCR machine after correcting the problem.
There may be more nonspecific bands in these PCR reactions than is typical either because there was a considerable delay waiting for all students to be ready to add their tubes to the PCR machine or because we had an issue where the program was initially incorrect and we needed to restart the PCR machine after correcting the problem.
-
Then we conducted a gel extraction, using QIAquick Gel Extraction Kit.
+
We cut the bands of the correct size out of the gel. Then we conducted a gel extraction, using QIAquick Gel Extraction Kit.
==Blunting the PCR Product==
==Blunting the PCR Product==
Line 40: Line 118:
After we had the purified PCR product, we used the Blunt Cloning Kit (NEB) to blunt and phosphorylate the ends of the PCR product. The blunting reaction was composed of:
After we had the purified PCR product, we used the Blunt Cloning Kit (NEB) to blunt and phosphorylate the ends of the PCR product. The blunting reaction was composed of:
-
Purified DNA: 15µl
+
:Purified DNA: 15µl
-
10X Blunting Buffer: 2.5µl
+
:10X Blunting Buffer: 2.5µl
-
1 mM dNTP Mix: 2.5µl
+
:1 mM dNTP Mix: 2.5µl
-
Blunt Enzyme Mix: 1.0µl
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:Blunt Enzyme Mix: 1.0µl
-
Sterile dH20: 4µl
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:Sterile dH20: 4µl
-
Total Volume: 25µl
+
:Total Volume: 25µl
Line 58: Line 136:
The pUC19 vector was digested with SmaI:
The pUC19 vector was digested with SmaI:
-
1µg/µl pUC19 (NEB): 5µl
+
:1µg/µl pUC19 (NEB): 5µl
-
10X NEBuffer 4: 3µl
+
:10X NEBuffer 4: 3µl
-
SmaI: 1 µl
+
:SmaI: 1 µl
-
H2O: 11 µl
+
:H2O: 11 µl
The restriction digest was incubated for 4 hours at 25°C. 1µl of Calf Intestinal Phosphatase (NEB) was added and the mixture was incubated at 37°C for 2 hrs.  
The restriction digest was incubated for 4 hours at 25°C. 1µl of Calf Intestinal Phosphatase (NEB) was added and the mixture was incubated at 37°C for 2 hrs.  
 +
 +
 +
[[Image:Dalton_Fig12.jpg]]
==Ligation==
==Ligation==
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==Transformation==
==Transformation==
-
For the transformation, we used NEB 10-beta Competent E. coli cells (cat # C3019H). We followed the manufacturer's suggested protocol for the transformation, and we plated on Ampicillin/IPTG/X-Gal.
+
For the transformation, we used NEB 10-beta Competent E. coli cells (cat # C3019H). We followed the manufacturer's suggested protocol for the transformation, and we plated on LB/Ampicillin/IPTG/X-Gal.
==BsaI-digested Miniprep DNA ==
==BsaI-digested Miniprep DNA ==
Overall, most plates contained a mixture of blue and white colonies and the number of colonies was fairly low - not much higher than for our "no insert" ligations.
Overall, most plates contained a mixture of blue and white colonies and the number of colonies was fairly low - not much higher than for our "no insert" ligations.
-
We then picked two white colonies from each plate and inoculated 2ml of LB/amp and then mini-prepped the DNA. Blue colonies had intact lacZ genes, and therefore did not contain inserts. The samples on these gels contain BsaI-digested miniprep DNA prepared from individual colonies from the transformations above.
+
We then picked two white colonies from each plate and inoculated 2ml of LB/amp and then mini-prepped the DNA. Blue colonies had intact lacZ genes, and therefore did not contain inserts. The samples on these gels contain BsaI-digested miniprep DNA prepared from individual white colonies from the transformations above.
For the BsaI Digest, we used:
For the BsaI Digest, we used:
-
Miniprep DNA: 4µl
+
:Miniprep DNA: 4µl
-
10X NEB4: 2µl
+
:10X NEB4: 2µl
-
100X BSA: .2µl
+
:100X BSA: .2µl
-
BsaI: .5µl
+
:BsaI: .5µl
-
H20: 13.3µl
+
:H20: 13.3µl
Line 98: Line 179:
pUC19 (no insert): 1 cut, 1 band: 2686 bp
pUC19 (no insert): 1 cut, 1 band: 2686 bp
-
pUC19 + insert: 3 cuts, 3 bands: 1354 bp, 1332 bp, insert (expected sizes listed on gel below)
+
pUC19 + insert: 3 cuts, 3 bands: 1354 bp, 1332 bp, insert (expected sizes listed on gel below).
 +
Almost all inserts are a single BsaI fragment, but there is an internal BsaI site in the TEF1, ENO1, EAF6, and MSN4 promoters so 2 band sizes are listed for these inserts.
Note that the 1354bp and 1332bp bands will appear to run as one band on the gel.
Note that the 1354bp and 1332bp bands will appear to run as one band on the gel.
Line 108: Line 190:
'''Promoters'''
'''Promoters'''
-
MET15    yes: B
+
:MET15    yes: B
-
GAL1    yes: A
+
:GAL1    yes: A
-
GAL1-L    yes: A
+
:GAL1-L    yes: A
-
GAL1-S    yes: B
+
:GAL1-S    yes: B
-
RAD52    yes: B
+
:RAD52    yes: B
-
RAD50    yes: A
+
:RAD50    yes: A
-
RAD54    yes: A, B
+
:RAD54    yes: A, B
-
RAD55    yes: A, B
+
:RAD55    yes: A, B
-
MRE11    yes: A, B
+
:MRE11    yes: A, B
-
XRS2    yes: A, B
+
:XRS2    yes: A, B
-
REV1    yes: B
+
:REV1    yes: B
-
TDH3    yes: A, B
+
:TDH3    yes: A, B
-
LIF1    '''none'''
+
:LIF1    '''none'''
-
MIG1    yes: B
+
:MIG1    yes: B
-
TUB1    yes: A
+
:TUB1    yes: A
-
CSE4    yes: B
+
:CSE4    yes: B
-
CLN2    yes: B
+
:CLN2    yes: B
-
CLB2    '''none'''
+
:CLB2    '''none'''
-
ACT1    '''none'''
+
:ACT1    '''none'''
-
ENO1    '''none'''
+
:ENO1    yes: A (we initially forgot there should be 2 insert bands and so continued to try to get clones in the next steps)
-
ENO2    '''none'''
+
:ENO2    '''none'''
-
TEF2    yes: B
+
:TEF2    yes: B
-
TEF1    '''none'''
+
:TEF1    '''none'''
-
EAF6    '''none''' (possibly a band, but too little DNA to be confident)
+
:EAF6    '''none''' (possibly a band, but too little DNA to be confident)
-
HSP12    yes: A, B
+
:HSP12    yes: A, B
-
HSP26    yes: A
+
:HSP26    yes: A
-
HSC82    '''none'''
+
:HSC82    '''none'''
-
MSN2    yes: A
+
:MSN2    yes: A
-
MSN4    '''none'''
+
:MSN4    '''none'''
-
HHO1    yes: A, D
+
:HHO1    yes: A, D
'''Protein-coding sequences'''
'''Protein-coding sequences'''
-
BFP    maybe: A (the insert may be too large)
+
:BFP    maybe: A (the insert may be too large)
-
GFP    '''none'''
+
:GFP    '''none'''
-
YFP    '''none'''
+
:YFP    '''none'''
-
mTangerine    '''none'''
+
:mTangerine    '''none'''
-
mCherry    yes: A (but bottom band seems possibly too intense)
+
:mCherry    yes: A (but bottom band seems possibly too intense)
-
mGrape1    '''none'''
+
:mGrape1    '''none'''
Line 191: Line 273:
DNA from these clones was miniprepped using Qiagen minipreps. The DNA was digested with BsaI as follows:
DNA from these clones was miniprepped using Qiagen minipreps. The DNA was digested with BsaI as follows:
-
miniprep DNA: 3µl
+
:miniprep DNA: 3µl
-
10X NEBuffer 4: 2µl
+
:10X NEBuffer 4: 2µl
-
100X BSA: 0.2µl
+
:100X BSA: 0.2µl
-
BsaI: 0.5µl
+
:BsaI: 0.5µl
-
H2O: 14.8µl
+
:H2O: 14.8µl
BsaI digests were incubated at 37°C for 2 hrs and then run on a 2% agarose gel in 1X sodium borate buffer.
BsaI digests were incubated at 37°C for 2 hrs and then run on a 2% agarose gel in 1X sodium borate buffer.
Line 211: Line 293:
'''Promoters'''
'''Promoters'''
-
LIF1    '''none'''
+
:LIF1    '''none'''
-
CLB2    yes: C
+
:CLB2    yes: C
-
ACT1    yes: C
+
:ACT1    yes: C
-
ENO1    '''none'''
+
:ENO1    '''none'''
-
ENO2    yes: C
+
:ENO2    yes: C
-
TEF1    '''none'''
+
:TEF1    '''none'''
-
EAF6    yes: D (This was started from culture EAF6-B)
+
:EAF6    yes: D (This was started from culture EAF6-B)
-
HSC82    '''none'''
+
:HSC82    '''none'''
-
MSN4    '''none'''
+
:MSN4    yes: C (we initially forgot there should be 2 insert bands and so continued to try to get clones in the next steps)
==Obtaining the remaining clones ==
==Obtaining the remaining clones ==
Line 234: Line 316:
1. Repeat the original blunt ligations using a higher insert:vector ratio.
1. Repeat the original blunt ligations using a higher insert:vector ratio.
-
2. Try a sticky-end ligation strategy since it may have a higher success rate than the blunt ligation strategy. (This strategy is outlined in detail below:
+
 
 +
2. Try a sticky-end ligation strategy since it may have a higher success rate than the blunt ligation strategy. This strategy is outlined in detail below:
When we designed the PCR primers, we added nucleotides 5' to the BSA recognition site in both the forward and reverse primers. We decided to introduce the sequence 5' CCCGGG 3'which is the site for both SmaI (creates blunt ends) and XmaI (creates sticky ends). According to the NEB catalog, SmaI and XmaI can cut very close to the end of a PCR product. Thus, the introduction served as a backup strategy if the blunt cloning was problematic. The PCR products could be cut with XmaI and ligated into XmaI-digested pUC19.
When we designed the PCR primers, we added nucleotides 5' to the BSA recognition site in both the forward and reverse primers. We decided to introduce the sequence 5' CCCGGG 3'which is the site for both SmaI (creates blunt ends) and XmaI (creates sticky ends). According to the NEB catalog, SmaI and XmaI can cut very close to the end of a PCR product. Thus, the introduction served as a backup strategy if the blunt cloning was problematic. The PCR products could be cut with XmaI and ligated into XmaI-digested pUC19.
 +
 +
 +
 +
[[Image:Dalton_Fig14.jpg]]
 +
 +
The original PCR reaction was digested with XmaI for the following promoters:
The original PCR reaction was digested with XmaI for the following promoters:
Line 243: Line 332:
-
purified PCR product: 15µl
+
:purified PCR product: 15µl
-
10X NEBuffer 4: 3µl
+
:10X NEBuffer 4: 3µl
-
100X BSA: 0.3µl
+
:100X BSA: 0.3µl
-
XmaI: 0.5µl
+
:XmaI: 0.5µl
-
H2O: 11.2µl
+
:H2O: 11.2µl
These digested PCR products were run on the gel below:
These digested PCR products were run on the gel below:
Line 266: Line 355:
-
5ng/µl fluorescent protein vector: 2µl
+
:5ng/µl fluorescent protein vector: 2µl
-
2X OneTaq Mix (NEB): 25µl
+
:2X OneTaq Mix (NEB): 25µl
-
5µM Forward primer: 2.5µl
+
:5µM Forward primer: 2.5µl
-
5µM Reverse primer: 2.5µl
+
:5µM Reverse primer: 2.5µl
-
H2O: 18µl
+
:H2O: 18µl
 +
 
 +
 
 +
'''Cycling conditions'''
 +
 
 +
:1 cycle of:
 +
 
 +
::94°C 5 min
 +
 
 +
:15 cycles of:
 +
 
 +
::94°C 30 sec
 +
 
 +
::50°C 30 sec
 +
 
 +
::68°C 45 sec
 +
 
 +
:30 cycles of:
 +
 
 +
::94°C 30 sec
 +
 
 +
::55°C 30 sec
 +
 
 +
::68°C 45 sec
 +
 
 +
:1 cycle of:
 +
 
 +
::68°C 5 min
Line 282: Line 398:
The purified PCR products were then digested with XmaI:
The purified PCR products were then digested with XmaI:
-
purified PCR product: 15µl
+
:purified PCR product: 15µl
-
10X NEBuffer 4: 3µl
+
:10X NEBuffer 4: 3µl
-
100X BSA: 0.3µl
+
:100X BSA: 0.3µl
-
XmaI: 0.5µl
+
:XmaI: 0.5µl
-
H2O: 11.2µl
+
:H2O: 11.2µl
These digested PCR products were run on the gel below and the bands were excised and purified using the QiaQuick Gel Extraction Kit.
These digested PCR products were run on the gel below and the bands were excised and purified using the QiaQuick Gel Extraction Kit.
Line 297: Line 413:
The pUC19 vector was digested with XmaI:
The pUC19 vector was digested with XmaI:
-
1µg/µl pUC19 (NEB): 5µl
+
:1µg/µl pUC19 (NEB): 5µl
-
10X NEBuffer 4: 3µl
+
:10X NEBuffer 4: 3µl
-
100X BSA: 0.3µl
+
:100X BSA: 0.3µl
-
XmaI: 0.5µl
+
:XmaI: 0.5µl
-
H2O: 11.2µl
+
:H2O: 11.2µl
The pUC19 vector was digested overnight at 37°C. Then, the reaction was heated at 65°C for 20min. 1µl of Calf Intestinal Phosphatase (NEB) was added to the reaction and it was incubated at 37°C for 2 hrs.  This digested, dephosphorylated vector was run on the agarose gel below.
The pUC19 vector was digested overnight at 37°C. Then, the reaction was heated at 65°C for 20min. 1µl of Calf Intestinal Phosphatase (NEB) was added to the reaction and it was incubated at 37°C for 2 hrs.  This digested, dephosphorylated vector was run on the agarose gel below.
Line 320: Line 436:
-
5µl of ligation reaction were transformed and plated on LB/Amp/X-gal/IPTG.  
+
5µl of ligation reaction were transformed and 150µl of the transformation was plated on LB/Amp/X-gal/IPTG.  
 +
 
 +
After about 18hrs, the plates with promoter clones had normal-sized colonies, but the colonies on the plates for the fluorescent protein coding sequences were just barely visible. We realized in retrospect that we probably shouldn't have plated the cells for the fluorescent protein sequences on IPTG/X-gal plates. The IPTG induced transcription of B-galactosidase with the fluorescent protein insertion. We know from previous experience with fluorescent protein plasmids that these proteins are somewhat toxic. The toxicity of the fluorescent proteins could explain the small size of the colonies. We would suggest not using blue/white selection for future cloning of protein-coding sequences. These fluorescent protein plates were allowed to grow 2 more days at room temperature before colonies were picked (2 days because we couldn't access the school building on a Sunday). We picked 2 colonies from each plate into LB/amp and miniprepped the DNA. Several of the colonies that we picked from the blunt cloning plates for the fluorescent proteins failed to grow in LB/amp.
 +
 
 +
BsaI digests to check the clones:
 +
 
 +
:miniprep DNA: 3µl
 +
 
 +
:10X NEBuffer 4: 2µl
 +
 
 +
:100X BSA: 0.2µl
 +
 
 +
:BsaI: 0.2µl
 +
 
 +
:H2O: 14.6µl
 +
 
 +
BsaI digests were incubated at 37°C overnight and then run on a 2% agarose gel (promoters) or 1% agarose gel (fluorescent protein coding sequences) in 1X sodium borate buffer.
 +
 
 +
 
 +
 
 +
[[Image:Dalton_Fig13.jpg]]
 +
 
 +
Based on the data above, we concluded that the following clones had inserts of the correct size:
 +
 
 +
'''Promoters'''
 +
 
 +
:LIF1    yes: X2
 +
 
 +
:ENO1    yes: X1,X2,B1,B2
 +
 
 +
:TEF1    yes: X1,X2,B1
 +
 
 +
:HSC82    yes: X1,X2,B1,B2
 +
 
 +
:MSN4    yes: X2,B1,B2
 +
 
 +
 
 +
'''Protein-coding sequences'''
 +
 
 +
:BFP    yes: X1,X2
 +
 
 +
:GFP    yes: X1,X2
 +
 
 +
:YFP    yes: X1,X2
 +
 
 +
:mTangerine    yes: X1,X2, B2
 +
 
 +
:mCherry    yes: X2
 +
 
 +
:mGrape1    yes: X1,X2
 +
 
 +
NOW WE HAVE ALL THE CLONES!!!
Return to our [https://2012hs.igem.org/Team:Dalton_School_NY main page].
Return to our [https://2012hs.igem.org/Team:Dalton_School_NY main page].

Latest revision as of 22:55, 6 June 2012

Contents

Testing of DNA prepared by several methods

Yeast genomic DNA is commonly prepared using a phenol/chloroform based method. Because both phenol and chloroform are toxic chemicals, we tested several methods for preparing yeast genomic DNA that do not use these chemicals. We compared a method that uses lithium acetate (LiOAc) to disrupt the yeast cell wall ([http://www.biotechniques.com/multimedia/archive/00147/BTN_A_000113672_O_147315a.pdf BioTechniques 50:325-328, 2011]) to methods that use the enzyme zymolyase to disrupt the cell wall (a Promega kit or a [http://www.bio.brandeis.edu/haberlab/jehsite/pdfs/ZymoPrep.pdf protocol from Jim Haber’s lab], “JH zym”). For the Haber lab protocol, we did not include beta mercaptoethanol (also toxic) in the zymolyase solution, realizing that without this the zymolyase step might take longer. We used the procedure in the Haber lab protocol to check the completion of the zymolyase digestion for the Promega protocol and the Haber lab protocol. DNA from all protocols was treated with RNase A. The Haber lab protocol produced the greatest yield of genomic DNA, but DNA made using the Promega kit was used in subsequent PCRs because it seemed to produce the most consistent results. 1µl, 2µl, or 5µl of genomic DNA was used in each PCR reaction with LIF1 promoter primers. The exception was that the DNA prepared using the Haber lab protocol was diluted 1:10 because it was about 10X more concentrated than the DNA prepared using the other methods. Following these initial tests, 1µl of yeast genomic DNA was used for subsequent PCRs. The LiOAc method was the shortest and least expensive and we may switch to this method when future DNA preps for PCR are needed. It should be noted that in retrospect, the PCR reactions below were too robust to fairly compare the DNA preps. DNA would need to be diluted and/or the cycles would need to be shortened to come close to having PCR reactions in the linear range. However, we learned from this that we had successfully prepared genomic DNA, so we moved forward.


For PCR, we used:

Yeast Genomic DNA: 1µl or 2µl or 5µl
2X OneTaq Mix (NEB): 25µl
5µM Forward primer: 2.5µl
5µM Reverse primer: 2.5µl
H2O: 19µl or 18µl or 15µl


Cycling conditions

1 cycle of:
94°C 5 min
15 cycles of:
94°C 30 sec
50°C 30 sec
68°C 45 sec
30 cycles of:
94°C 30 sec
55°C 30 sec
68°C 45 sec
1 cycle of:
68°C 5 min

2% agarose gels in 1X Sodium Borate buffer: [http://www.biotechniques.com/multimedia/archive/00036/BTN_A_04362BM02_O_36180a.pdf BioTechniques 36:214-216 (February 2004)]

"LiOAc (liq)" = Lithium acetate, prepped from yeast in liquid culture

"LiOAc (col)" = Lithium acetate, prepped from a yeast colony

"JH zym" = Prepped with Haber lab zymolyase protocol

"Promega" = Prepped with Promega Wizard Genomic DNA kit

Dalton Fig7.jpg

PCR of promoters and fluorescent protein coding sequences

We did an isolation of genomic DNA from yeast using the Promega Wizard Genomic DNA Purification Kit- cat# A1120. We substituted 20T zymolyase (Seikagaku) for lyticase and monitored the zymolyase digestion for completion.

PCR primers were designed by students and supplied by IDT.


For PCR, we used:

Yeast Genomic DNA: 1µl OR 1µl of 5ng/µl fluorescent protein plasmid
2X OneTaq Mix (NEB): 25µl
5µM Forward primer: 2.5µl
5µM Reverse primer: 2.5µl
H2O: 19µl


Cycling conditions

1 cycle of:
94°C 5 min
15 cycles of:
94°C 30 sec
50°C 30 sec
68°C 45 sec
30 cycles of:
94°C 30 sec
55°C 30 sec
68°C 45 sec
1 cycle of:
68°C 5 min


The ladder on all gels is the 2-log ladder (NEB).

2% agarose gels in 1X Sodium Borate buffer: [http://www.biotechniques.com/multimedia/archive/00036/BTN_A_04362BM02_O_36180a.pdf BioTechniques 36:214-216 (February 2004)]

Dalton Fig6.jpg

There may be more nonspecific bands in these PCR reactions than is typical either because there was a considerable delay waiting for all students to be ready to add their tubes to the PCR machine or because we had an issue where the program was initially incorrect and we needed to restart the PCR machine after correcting the problem.

We cut the bands of the correct size out of the gel. Then we conducted a gel extraction, using QIAquick Gel Extraction Kit.

Blunting the PCR Product

After we had the purified PCR product, we used the Blunt Cloning Kit (NEB) to blunt and phosphorylate the ends of the PCR product. The blunting reaction was composed of:

Purified DNA: 15µl
10X Blunting Buffer: 2.5µl
1 mM dNTP Mix: 2.5µl
Blunt Enzyme Mix: 1.0µl
Sterile dH20: 4µl
Total Volume: 25µl


Digestion of pUC19

The pUC19 vector was digested with SmaI:

1µg/µl pUC19 (NEB): 5µl
10X NEBuffer 4: 3µl
SmaI: 1 µl
H2O: 11 µl

The restriction digest was incubated for 4 hours at 25°C. 1µl of Calf Intestinal Phosphatase (NEB) was added and the mixture was incubated at 37°C for 2 hrs.


Dalton Fig12.jpg

Ligation

Next, we did a ligation reaction with the Quick Ligation Kit (NEB). We followed the manufacturer's suggested protocol which was to use a 3:1 molar ratio of insert: vector and 50 ng of SmaI digested/CIP'd pUC19 vector.

Transformation

For the transformation, we used NEB 10-beta Competent E. coli cells (cat # C3019H). We followed the manufacturer's suggested protocol for the transformation, and we plated on LB/Ampicillin/IPTG/X-Gal.

BsaI-digested Miniprep DNA

Overall, most plates contained a mixture of blue and white colonies and the number of colonies was fairly low - not much higher than for our "no insert" ligations. We then picked two white colonies from each plate and inoculated 2ml of LB/amp and then mini-prepped the DNA. Blue colonies had intact lacZ genes, and therefore did not contain inserts. The samples on these gels contain BsaI-digested miniprep DNA prepared from individual white colonies from the transformations above.

For the BsaI Digest, we used:

Miniprep DNA: 4µl
10X NEB4: 2µl
100X BSA: .2µl
BsaI: .5µl
H20: 13.3µl


Expected band sizes from BsaI digests

pUC19 (no insert): 1 cut, 1 band: 2686 bp

pUC19 + insert: 3 cuts, 3 bands: 1354 bp, 1332 bp, insert (expected sizes listed on gel below). Almost all inserts are a single BsaI fragment, but there is an internal BsaI site in the TEF1, ENO1, EAF6, and MSN4 promoters so 2 band sizes are listed for these inserts.

Note that the 1354bp and 1332bp bands will appear to run as one band on the gel.

Dalton Fig8.jpg

Based on the data above, we concluded that the following clones had inserts of the correct size:

Promoters

MET15 yes: B
GAL1 yes: A
GAL1-L yes: A
GAL1-S yes: B
RAD52 yes: B
RAD50 yes: A
RAD54 yes: A, B
RAD55 yes: A, B
MRE11 yes: A, B
XRS2 yes: A, B
REV1 yes: B
TDH3 yes: A, B
LIF1 none
MIG1 yes: B
TUB1 yes: A
CSE4 yes: B
CLN2 yes: B
CLB2 none
ACT1 none
ENO1 yes: A (we initially forgot there should be 2 insert bands and so continued to try to get clones in the next steps)
ENO2 none
TEF2 yes: B
TEF1 none
EAF6 none (possibly a band, but too little DNA to be confident)
HSP12 yes: A, B
HSP26 yes: A
HSC82 none
MSN2 yes: A
MSN4 none
HHO1 yes: A, D


Protein-coding sequences

BFP maybe: A (the insert may be too large)
GFP none
YFP none
mTangerine none
mCherry yes: A (but bottom band seems possibly too intense)
mGrape1 none


Extra colonies were picked from the transformations for the following promoter clones:

LIF1, CLB2, ACT1, ENO1, ENO2, TEF1, EAF6, HSC82, MSN4

DNA from these clones was miniprepped using Qiagen minipreps. The DNA was digested with BsaI as follows:

miniprep DNA: 3µl
10X NEBuffer 4: 2µl
100X BSA: 0.2µl
BsaI: 0.5µl
H2O: 14.8µl

BsaI digests were incubated at 37°C for 2 hrs and then run on a 2% agarose gel in 1X sodium borate buffer.


Dalton Fig9.jpg


Based on the data above, we concluded that the following clones had inserts of the correct size:

Promoters

LIF1 none
CLB2 yes: C
ACT1 yes: C
ENO1 none
ENO2 yes: C
TEF1 none
EAF6 yes: D (This was started from culture EAF6-B)
HSC82 none
MSN4 yes: C (we initially forgot there should be 2 insert bands and so continued to try to get clones in the next steps)

Obtaining the remaining clones

Because there had been relatively few colonies on most of the transformation plates, we decided to try 2 different strategies for obtaining the remaining clones:

1. Repeat the original blunt ligations using a higher insert:vector ratio.

2. Try a sticky-end ligation strategy since it may have a higher success rate than the blunt ligation strategy. This strategy is outlined in detail below:

When we designed the PCR primers, we added nucleotides 5' to the BSA recognition site in both the forward and reverse primers. We decided to introduce the sequence 5' CCCGGG 3'which is the site for both SmaI (creates blunt ends) and XmaI (creates sticky ends). According to the NEB catalog, SmaI and XmaI can cut very close to the end of a PCR product. Thus, the introduction served as a backup strategy if the blunt cloning was problematic. The PCR products could be cut with XmaI and ligated into XmaI-digested pUC19.


Dalton Fig14.jpg


The original PCR reaction was digested with XmaI for the following promoters:

LIF1, ENO1, TEF1, HSC82, MSN4


purified PCR product: 15µl
10X NEBuffer 4: 3µl
100X BSA: 0.3µl
XmaI: 0.5µl
H2O: 11.2µl

These digested PCR products were run on the gel below:

2% agarose gel in 1X sodium borate buffer:

Dalton Fig10.jpg

These bands were excised and purified using the QiaQuick Gel Extraction Kit.


Because the cloning of the fluorescent proteins was particularly problematic, we repeated the PCR of these genes:


5ng/µl fluorescent protein vector: 2µl
2X OneTaq Mix (NEB): 25µl
5µM Forward primer: 2.5µl
5µM Reverse primer: 2.5µl
H2O: 18µl


Cycling conditions

1 cycle of:
94°C 5 min
15 cycles of:
94°C 30 sec
50°C 30 sec
68°C 45 sec
30 cycles of:
94°C 30 sec
55°C 30 sec
68°C 45 sec
1 cycle of:
68°C 5 min


PCR products were purified using the QiaQuick Gel Extraction Kit.


The purified PCR products were then digested with XmaI:

purified PCR product: 15µl
10X NEBuffer 4: 3µl
100X BSA: 0.3µl
XmaI: 0.5µl
H2O: 11.2µl

These digested PCR products were run on the gel below and the bands were excised and purified using the QiaQuick Gel Extraction Kit.


The pUC19 vector was digested with XmaI:

1µg/µl pUC19 (NEB): 5µl
10X NEBuffer 4: 3µl
100X BSA: 0.3µl
XmaI: 0.5µl
H2O: 11.2µl

The pUC19 vector was digested overnight at 37°C. Then, the reaction was heated at 65°C for 20min. 1µl of Calf Intestinal Phosphatase (NEB) was added to the reaction and it was incubated at 37°C for 2 hrs. This digested, dephosphorylated vector was run on the agarose gel below.

2% agarose gel in 1X sodium borate buffer:

Dalton Fig11.jpg

These bands were excised and purified using the QiaQuick Gel Extraction Kit.

Strategy 1: blunted PCR products were ligated into SmaI/CIP'd pUC19 vector as before, except that a 10:1 molar insert:vector ratio was used.

Strategy 2: XmaI-digested PCR products were ligated into XmaI/CIP'd pUC19 vector using a 6:1 molar insert:vector ratio.


5µl of ligation reaction were transformed and 150µl of the transformation was plated on LB/Amp/X-gal/IPTG.

After about 18hrs, the plates with promoter clones had normal-sized colonies, but the colonies on the plates for the fluorescent protein coding sequences were just barely visible. We realized in retrospect that we probably shouldn't have plated the cells for the fluorescent protein sequences on IPTG/X-gal plates. The IPTG induced transcription of B-galactosidase with the fluorescent protein insertion. We know from previous experience with fluorescent protein plasmids that these proteins are somewhat toxic. The toxicity of the fluorescent proteins could explain the small size of the colonies. We would suggest not using blue/white selection for future cloning of protein-coding sequences. These fluorescent protein plates were allowed to grow 2 more days at room temperature before colonies were picked (2 days because we couldn't access the school building on a Sunday). We picked 2 colonies from each plate into LB/amp and miniprepped the DNA. Several of the colonies that we picked from the blunt cloning plates for the fluorescent proteins failed to grow in LB/amp.

BsaI digests to check the clones:

miniprep DNA: 3µl
10X NEBuffer 4: 2µl
100X BSA: 0.2µl
BsaI: 0.2µl
H2O: 14.6µl

BsaI digests were incubated at 37°C overnight and then run on a 2% agarose gel (promoters) or 1% agarose gel (fluorescent protein coding sequences) in 1X sodium borate buffer.


Dalton Fig13.jpg

Based on the data above, we concluded that the following clones had inserts of the correct size:

Promoters

LIF1 yes: X2
ENO1 yes: X1,X2,B1,B2
TEF1 yes: X1,X2,B1
HSC82 yes: X1,X2,B1,B2
MSN4 yes: X2,B1,B2


Protein-coding sequences

BFP yes: X1,X2
GFP yes: X1,X2
YFP yes: X1,X2
mTangerine yes: X1,X2, B2
mCherry yes: X2
mGrape1 yes: X1,X2


NOW WE HAVE ALL THE CLONES!!!


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