Contents 1 Agilent's Pointmutation method 1.1 PCR reaction 1.2 DpnI digestion 1.3 Nanodrop test after digestion 1.4 Bacteria transformation 1.5 Gel electrophoresis 2 Agilent's Pointmutation method II 2.1 PCR 2.2 Nanodrop test 2.3 Gel electrophoresis 3 2-pair primers PCR 3.1 PCR 3.2 Gel electrophoresis 3.3 PCR II 3.4 Gel electrophoresis: 4 2-pari primers PCR II 4.1 PCR 4.2 Gel electrophoresis 4.3 Gel electrophoresis II 5 Half-plasmid PCR & Double primer PCR 5.1 Half-plasmid PCR 5.2 Double primer PCR 5.3 Gel electrophoresis 5.4 Gel extraction 5.5 Nanodrop test 5.6 BbsI enzyme digestion 5.7 Gel electrophoresis 6 Verification of the Point mutation 6.1 Enzyme Digestion 6.1.1 BbsI, BspEI double digestion(10:05~21:30) 6.1.2 BspEI digestion (15:41~21:30) 6.2 Gel electrophoresis 6.3 Gel electrophoresis II 7 References

By Yicong Tao

Plasmid used: pBX-084 PB5-HS4-TRE-mCherrynuc-2A-BlaloxN-GpA-HS4-PB3 (from Wei Huang’s lab). Total length is 6843bp.

Point mutation primer design:
Forward(5’-3’): cagcccatggttttcttctgcattacggggccg 33nt
Reverse(5’-3’): cggccccgtaatgcagaagaaaaccatgggctg 33nt
The primer pair is intended to eliminate the BbsI site in the mCherry because we need to use BbsI to insert our gRNA into our plasmid. Designed by Agilent Technologies point-mutation primer online design tools. The primers are complement with each other.

Agilent's Pointmutation method

8.13~8.14

PCR reaction

(12:06~14:XX 13th Aug, about 2h)

300ul, 50ul/reaction:

Component	Volume	Final Concentration
Q5 master mix 2X	150ul	1X
DNA template (251.4ng/ul)	1.5ul	1.257ng/ul
Primer F (50uM)	3ul	500nM
Primer R (50uM)	3ul	500nM
ddH20	142.5ul	-
Total	300ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
18 cycles	98	10
58, 60, 61, 62, 63, 65	15
72	360
Final extension	72	120
Hold	4	∞

DpnI digestion

(13 Aug 15:05~19:06)

Add 1ul DpnI directly to the amplification system

Digest 4h

No termination

Stored at -20℃

Nanodrop test after digestion

Anneal Temp (℃)	58	60	61	62
Conc (ng/ul)	467.4	465.9	470.4	457.9
260/280	1.8	1.8	1.8	1.81
260/230	0.73	0.73	0.74	0.73

Bacteria transformation

(2014.8.13 22:08~2014.8.14 14:50)

Procedures:

1. Immediately, place the tubes on ice, allow cell to thaw on ice, 10 min
2. Check the cell to see if they have thawed, gently flick the cells 1-2 times to evenly resuspend the cells.
3. Divide the competent cells into 6 tubes,50μL each tube, Mark them with 58, 60, 61, 62, 63, 65. Keep the bacteria in ice during the procedure.
4. Add 5μL plasmid to each tube, shaking slightly
5. Incubate on ice for 30min
6. Heat shock, 42°C, 90s.
7. Keep on ice, 2 min
8. Add 200μl SOC medium to each tube, incubate 37°C, 200rpm, 45min
9. Centrifuge, 4000rmp, 5min, RT. Discard most of the medium and reserve 50μL. Resuspend.
10. Add 50μL bacteria to amp LB agar plate, distribute.
11. Incubate the plates at 37°C, 16 hours.

Results:

For all 6 groups, no colony forms.

Gel electrophoresis

Making the agarose gel (1%)

Component	Volume
TAE	25ml
Agarose	0.25g
Gene Green	0.5ul

Adding samples

Component	Volume
PCR product	1ul
6X loading dye	2ul
TAE	9ul
Total	12ul

DNA marker (Takara DL5000, diluted): 10ul

Results:

The result of electrophoresis is not clear, so I redid the gel electrophoresis with the same sample.

No wanted band (6843bp) is observed.

Discussion:

1. PCR failed, so improving PCR conditions is the first choice. Try extending PCR cycles, denaturation time, annealing time and final extension time.
2. Do reaction termination after DpnI enzyme digestion (80℃ 20min) next time because reactive enzyme may binding to the DNA substrate and interfere the transformation efficiency.
3. The concentration of template DNA is also very essential, so using 2-step concentration ladder next time.

Agilent's Pointmutation method II

8.15

PCR

(23:35 14th Aug-08:30 15th Aug), about 2h. Next morning, check PCR machine was not at 4℃ hold conditions, and the heating stand was not cold
200ul, 50ul/reaction:

Component	Volume	Final Concentration
Q5 master mix 2X	100ul	1X
DNA template (251.4ng/ul)	1.0ul (A,B), 2.0ul (C,D)	1.257ng/ul (A,B), 2.514ng/ul (C,D)
Primer F (50uM)	2ul	500nM
Primer R (50uM)	2ul	500nM
ddH20	95ul	-
Total	200ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	63	30
	72	420
Final extension	72	600
Hold	4	∞

Nanodrop test

Anneal Temp (℃)	A	B	C	D
Conc (ng/ul)	474.2	492.0	466.7	445.9
260/280	1.82	1.81	1.81	1.81
260/230	0.72	0.73	0.72	0.70

Gel electrophoresis

Making the agarose gel (1%)

Component	Volume
TAE	25ml
Agarose	0.25g
Gene Green	0.5ul

Adding samples

Component	Volume
PCR product	5ul
6X loading dye	2ul
TAE	5ul
Total	12ul

DNA marker (Takara DL5000, diluted): 10ul

Results:

Analysis:
The band was in 2000bp location, which is far away from the original plasmid length (6800bp), which meant PCR didn’t got complete plasmid.
The possible reason might be:

1. The primer forms dimers which strongly influence the efficiency of PCR (The smallest band is very light).
2. DNA is a double helix, which means the plasmid double strand can also anneal with each other. The elongation time was very long, which left enough time for the plasmid double strand to anneal with each other and prohibit the PCR process.

Solution:

1. Redesign the primer so that the primer pairs are not totally complementary with each other. Put the point mutation point near the 5’ end.
2. Use other PCR methods.

So I decided to change the PCR method.

2-pair primers PCR

I had two pairs of primers: one is for mCherry (called A), another is for point mutation (called B). I then used the forward primer of A to pair with the reverse primer of B, so did the forward primer of B with the reverse primer of A. Thus, I would get 2 short segments which had a small complementary region. Then, I added the two segments together and let them do PCR using each other as the template and primer in order to get the final whole length PCR product.

mCherry primer design:
Forward(5’-3’): TCGTTTAGTGAACCGTCAG 19nt
Reverse(5’-3’): cgaggaattcctattaTTCCTCTGCCCTCACTAG 34nt

PCR

50ul, 25ul/reaction:
Reaction 1:

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	2.0ul	1.257ng/ul
mCherry Primer F (50uM)	0.5ul	500nM
Pointmutation Primer R (50uM)	0.5ul	500nM
ddH20	22ul	-
Total	50ul	-

Reaction 2:

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	2.0ul	1.257ng/ul
mCherry Primer R (50uM)	0.5ul	500nM
Pointmutation Primer F (50uM)	0.5ul	500nM
ddH20	22ul	-
Total	50ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	61	15
	72	20
Final extension	72	300
Hold	4	∞

Gel electrophoresis

Making the agarose gel (1%)

Component	Volume
TAE	25ml
Agarose	0.25g
Gene Green	0.5ul

Adding samples

Component	Volume
PCR product	10ul
6X loading dye	2ul
Total	12ul

DNA marker (Takara DL5000, diluted): 30ul

Results:
A2: reaction 1 (A: mCherry primer F; 2: Pointmutation Primer R)
1B: reaction 2 (B: mCherry primer R; 1: Pointmutation Primer F)

Analysis:
The predicting results is 448bp band in A2 and 372bp band in 1B (almost equally separate the mCherry). But the band in A2 was in 800bp and no band is observed in 1B. The possible reasons might be:

1. I added wrong primer pairs: two mCherry primers for A2 and two pointmutation primers for 1B. So that in A2 I got mCherry and in 1B I got primer dimer.
2. The elongation time might be too long.

So I redid the 2-pari primers PCR with modified PCR reaction conditions.

PCR II

Reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	61	15
	72	15
Final extension	72	120
Hold	4	∞

Gel electrophoresis:

Results:
No band is observed.
Analysis:

1. The elongation time might be too short…
2. The annealing time for 1B might be wrong.

2-pari primers PCR II

8.16 10:25am~11.25am
I set a temperature gradient (45, 48, 51, 54, 57, 60℃) without shortening the elongation time.

PCR

150ul, 25ul/reaction:
Reaction 1:

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	0.5ul	12.57ng
Pointmutation Primer F (50uM)	1ul	1000nM
ddH20	23ul	-
Total	49.5ul	-

Reaction 2:

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	0.5ul	12.57ng
Pointmutation Primer R (50uM)	1ul	1000nM
ddH20	23ul	-
Total	49.5ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	63	15
	72	5min
Final extension	72	10min
Hold	4	∞

Gel electrophoresis

11:50am ~12:25pm
Unfortunately, only in A2 did I observe the band. I doubt the annealing temperature was not high enough because strong primer dimers forms in 1B group. So I redid the 2-pair primers PCR again with even higher temperature gradient (62,63,64,65,66,67℃).

Gel electrophoresis II

Results:
Only vague bands were observed in A2. Still no distinct bands observed in 1B.
Analysis:

1. The reverse primer of pointmutation might be very easy to form dimer with the forward primer of mCherry, which led to the failure of PCR.
2. The compatibility of the two separate primers might be very bad.

I decided to try another methods.

Half-plasmid PCR & Double primer PCR

Half-plasmid PCR

First, only add one direction primer so I could get half linear plasmid. After that, I mix the two DNA together to get the complete DNA.
50ul, 25ul/reaction:
Reaction 1

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	0.5ul	12.57ng
Pointmutation Primer F (50uM)	1ul	1000nM
ddH20	23ul	-
Total	49.5ul	-

Reaction 2

Component	Volume	Final Concentration
Q5 master mix 2X	25ul	1X
pBX084 diluted (25.14ng/ul)	0.5ul	12.57ng
Pointmutation Primer R (50uM)	1ul	1000nM
ddH20	23ul	-
Total	49.5ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	63	15
	72	5min
Final extension	72	10min
Hold	4	∞

Double primer PCR

Mix the two pairs of primer together but the density of the pointmutation primer is only 1/10 of the mCherry primer. So the pointmutation primer will be consumed very quickly in the first several rounds.
150ul, 25ul/reaction:

Component	Volume	Final Concentration
Q5 master mix 2X	75ul	1X
pBX084 diluted (25.14ng/ul)	1ul	25.14ng
mCherry Primer F&R (50uM)	2ul	6666.7nM
Pointmutation Primer R (50uM)	0.2ul	666.7nM
ddH20	69.6ul	-
Total	150ul	-

PCR reaction conditions:

Step	Temp (℃)	Time (s)
Initial denaturation	98	60
25 cycles	98	20
	45,48,52,55,58,61	20
	72	20
Final extension	72	5min
Hold	4	∞

The two PCR methods proceed simultaneously from 17:00 to 19:30, then reserved in 4℃.

Gel electrophoresis

8.17 Analysis:
From Double-primer PCR we got 2 (or 3?) bands. The band which had length between 500~750 were very likely to be the successfully mutated (or the original template). The band between 250~500 might be the combination product of the two primer pairs.
Next I would do gel extraction for the 500~750 band and do BbsI enzyme digestion to verify if the BbsI site was successfully mutated or not.

Gel extraction

(13:53~15:20 Aug 15th) Tiangen Miniprep gel extraction kit (50 rxn)
As the Tiangen’s protocol instructed.

Nanodrop test

Band	700bp	400bp
Conc (ng/ul)	54.7	73.2
260/280	1.094	1.464
260/230	0.634	0.445

BbsI enzyme digestion

(15:50~20:00, 4h10min)

Component	Volume
NEB BbsI enzyme	0.2ul
DNA (700bp band)	3ul
10X NEB buffer 2.1	1ul
ddH20	5.8ul
Total	10ul

75℃ 20min inactivation in dry bath

Gel electrophoresis

(23:00~23:40)： Analysis:
After enzyme digestion, the band wasn’t cut into two bands (one about 440, another about 370).
The next day I would do BbsI and BspEI double digestion to verify the results because BspEI would cut out a 99bp band.
P.S. The expected band length is 820bp, which seems to be inconsistent with the figure. However, comparing with the PCR result of mCherry, the band location seems to be the same, which means it was likely to be the problem of Marker.

Verification of the Point mutation

8.18

Enzyme Digestion

BbsI, BspEI double digestion(10:05~21:30)

Component	Volume
BbsI	0.8ul
BspEI	0.2ul
700bp band	3ul
10X NEBuffer 3.1	1ul
ddH2O	5ul
Total	10ul

The activity of BbsI in NEBuffer 3.1 is only about 25%, so I increase the volumn the BbsI to 4X.

BspEI digestion (15:41~21:30)

Component	Volume
BbsI	0.2ul
700bp band	3ul
10X NEBuffer 3.1	1ul
ddH2O	5.8ul
Total	10ul

80℃ inactivation, then immediately put into ice to avoid self-ligation.(21:40~22:40）

Gel electrophoresis

(22:50~23:20) Analysis:
The DNA might decompose due to too long inactivation time (1h at 80℃).
However, Le Lin and Zeng Lidan thought high temp wouldn’t make DNA decompose. It was due to putting in ice immediately that makes DNA renaturation difficult.
So, I decided to do enzyme digestion again without heat inactivation and do gel electrophoresis to see the results. I also will put the enzyme digestion system into 4℃ refrigerator overnight and do gel electrophoresis again the next day to verify if Le and Zeng’s idea was correct.

Gel electrophoresis II

8.19 Analysis:
From the gel electrophoresis result, Lin and Zeng’s idea was not correct because again no band is observed. BspEI digestion cut off a 99bp short segment and we can see the band moved quicker than BbsI band. The 273bp band was not observed in BspEI & BbsI double digestion, which means no BbsI site is in the PCR product.

So the pointmutation was finally successful!!!

References

1. QuikChange Primer Design:[http://www.genomics.agilent.com/primerDesignProgram.jsp]
2. QuikChange II Site-Directed Mutagenesis Kits - Details & Specifications: [http://www.genomics.agilent.com/article.jsp?pageId=384]