Difference between revisions of "Team:NYU Abu Dhabi/Results"
| Line 1,035: | Line 1,035: | ||
</i></center></h2> | </i></center></h2> | ||
<br> | <br> | ||
| − | <h2>Confirming the hydrophilicity of the chip, a prototype made from double sided tape and film was tested. The chip had a channel width of | + | <h2>Confirming the hydrophilicity of the chip, a prototype made from double sided tape and film was tested. The chip had a channel width of 200µ m, which is a conventional width for PDMS microfluidic chip. However, the liquid did not flow to the wells. Through varying different width of the microfluidic chip, we realized that maximizing the surface area exposed to the hydrophilic film is more important than varying surface pressure of the wells. The finalized chip had a 600µm width to ensure good flow but prevent flowback. </h2> |
<br> | <br> | ||
<h7><ins>Amplification</ins></h7> | <h7><ins>Amplification</ins></h7> | ||
<br><br> | <br><br> | ||
| − | <h2>The reagents for two positive as well as two negative NEB LAMP reactions were added to four different wells on PDMS chip. Each reaction contained 12.5 & | + | <h2>The reagents for two positive as well as two negative NEB LAMP reactions were added to four different wells on PDMS chip. Each reaction contained 12.5µ l of mastermix, 9 µ l of water and 1µ l of miniprep DNA. Positive control reactions contained 2.5µ l of primers, while in negative control reactions, the same volume of water was added instead. After the reagents were added to the chip, it was covered with hydrophobic PCR tape in order to prevent evaporation of the reagents throughout the reactions.The reactions were then run for 30 minutes by placing the chip on a hot plate heated to a temperature of 65°C. Figure 1 shows the chip as viewed under blue light. The wells containing positive are marked with a + symbol while the negative controls are marked with a - symbol. |
</h2> | </h2> | ||
| Line 1,047: | Line 1,047: | ||
</i></center></h2> | </i></center></h2> | ||
<br> | <br> | ||
| − | <h2>Next, the four RPA reactions were carried out in a 3M chip. For one RPA reaction, 29.5 µ l of re-hydration buffer was added to one tube of dried reaction, along with 2.4 & | + | <h2>Next, the four RPA reactions were carried out in a 3M chip. For one RPA reaction, 29.5 µ l of re-hydration buffer was added to one tube of dried reaction, along with 2.4µ l forward primers, 2,4 µ l backward primers, 8.2µ l of water, 5µ l of DNA, 1µ l of 1000X SBYR Green and 2.5 µ l of Magnesium acetate. The primers were replaced with an equal volume of water for the two negative control reactions. |
</h2> | </h2> | ||
Revision as of 17:32, 17 October 2018
Results
The team started with performing PCR for the plasmids as it is a general technique and the results would serve as a standard to compare the results of LAMP and RPA, the other relatively new amplification techniques we used for the project.
We performed PCR, LAMP and RPA reactions to characterize our plasmids and determine if amplification happens with our designed primers. We wanted to test how specific each of these amplification techniques is by running each plasmid with its primers and the primers of other fragments. Our results show that LAMP is the most specific amplification technique which is consistent with results from the literature that show that LAMP has very high specificity (1). PCR had the lowest specificity which is also consistent with results from literature (2). RPA has been shown to be the best amplification technique currently available in terms of parameters like speed, complexity, and user-friendliness. However, our results show that RPA is less specific than LAMP. Daher et al (2015) (3) showed that mismatches can occur if extra precautions are not taken during primer design to eliminate this. In our case, our primers could be the reason for RPA being less specific than LAMP.
We also tested how sensitive LAMP and PCR are by checking for the lowest concentration of DNA past which amplification is lost. We visualized amplification for both techniques by gel electrophoresis. We visualized the results for LAMP alone by adding SYBR green to the reaction post-amplification and visualizing with UV light. The results show that both LAMP and PCR have a similar sensitivity of up to 0.1 ng/μl of DNA. however, results from literature (4)(5) have shown that LAMP is significantly more sensitive than PCR.
As we would be using SYBR green in our device for visualization of amplification, we performed experiments to determine the optimal concentration of SYBR green to be added to our LAMP reaction and the wavelength of UV light that allows for the best visualization. We found that 1000X SYBR green in 25 μl total volume of LAMP reactants visualized with 254 nm UV light gave the best results.
To test if the results obtained from intra-lab amplification using miniprep DNA would work in our device which would use samples of putatively contaminated food or water, we tested detection of lmo0733 gene from Listeria Monocytogenes in beef. Ground beef was spiked with lmo0733 and E. Coli (as control for specificity) and direct swabs of prepared beef samples were used to run a LAMP reaction using NEB WarmStart colorimetric mastermix and lmo0733 primers. We observed a distinct yellow color in reactions with samples spiked with lmo0733 15 minutes after the reaction which confirms amplification; while samples from unspiked beef (negative control) and beef grown with E. Coli remained bright red. Gel electrophoresis was also used to confirm the results of the colorimetric amplification.
PCR
PCR reactions were run with designed primers to confirm that the primers amplify the gene of interest and also characterize the DNA fragments we would be working with. The agarose gel (1%) shows bands at expected lengths for lmo0733 (430 bp), gbpA (1019 bp) and invA (818 bp). The negative controls show no bands i.e. no amplification which is what was expected. PCR reactions were run to test the specificity of the primers for this technique. Each gene was run with its primers and the primers of other gene fragments
Sensitivity (lmo0773, invA and hipO)
In order to determine the PCR reaction sensitivity, the reaction was run with serial dilutions of miniprepped plasmid with the gene of interest. The reactions were set up according to an optimized protocol used in the laboratory.
Figure 1. Agarose gels (1%) corresponding to the PCR reaction with serial dilutions of miniprepped lmo0773, invA and hipO DNA. (a). lmo0773 serial dilutions 363 ng/µl, 200 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl. (b). invA serial dilutions 295.5 ng/µl, 200 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl. (c). hipO serial dilutions 159.8 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl
Results obtained clearly shows that PCR is sensitive up to 0.1 ng/µl, lowest concentration tested, for all three plasmids tested. Visually, all bands appear to be similarly thick, which shows that, despite the changes in concentration, PCR amplified each DNA in a similar manner.
Published research has reported PCR to be sensitive up to 3 pg/µl (6). This shows that PCR is a sensitive technique that is able to amplify DNA even at low DNA concentrations.
Specificity (lmo0773, invA and gbpA)
Two sets of experiments were carried out to test the specificity of each amplification technique used. In the first set of experiments, the genes used were kept constant, while the primers were varied, while in the second set, the primers were kept constant while the genes were varied. As can be seen in the figure below, PCR was not found to be specific, as the DNA for a specific gene was amplified by primers designed for another gene as well as with primers specific for that gene.
Figure 2. Agarose gels (1%) corresponding to PCR specificity reactions carried out on three different genes (a) lmo0733, (b) invA and (c) hipO. The first set of reactions for each gene is done by keeping the gene constant while varying the primers, while the second set of reactions are carried out by varying the gene used while keeping the primers constant.
LAMP
Loop-mediated isothermal amplification was performed using primers designed with PrimerExplorer for lmo0733, invA, hipO and gbpA. The reaction was run using miniprep DNA and transformed E. Coli colonies to assess if amplification can occur with whole cells. The Agarose gel (1%) shows amplification in all the lanes with miniprep DNA.
Figure 3. Agarose gel (1%) showing LAMP amplification of invA, gbpA and lmo0733 miniprep DNA with designed LAMP primers (PrimerExplorer). Amplification is seen for lmo0733 and gbpA but not invA when gene transformed E. Coli colonies were used. (Lane 1) 500 bp ladder; (Lane 2) invA miniprep + invA LAMP primers; (Lane 3) Nuclease-free water + invA LAMP primers; (Lane 4) invA transformed E. Coli colony + invA LAMP primers; (Lane 5) gbpA miniprep + gbpA LAMP primers; (Lane 6) Nuclease-free water + gbpA LAMP primers; (Lane 7) gbpA transformed E. Coli colony + gbpA LAMP primers; (Lane 8) lmo0733 miniprep + lmo0733 LAMP primers; (Lane 9) Nuclease-free water + lmo0733 LAMP primers; (Lane 10) lmo0733 transformed E. Coli colony + lmo0733 LAMP primers.
Figure 4. Agarose gel (1%) showing LAMP amplification of gbpA with non colorimetric reaction mastermix (MM) (Optigene) with either hydroxy naphthol blue (HNB) or SYBR green added and with colorimetric reaction mastermix (NEB). (Lane 1) 500 bp ladder; (Lane 2) gbpA + Optigene MM + gbpA LAMP primers + HNB; (Lane 3) nuclease free water + Optigene MM + gbpA primers + HNB; (Lane 4) gbpA + Optigene MM + gbpA LAMP primers + SYBR green; (Lane 5) Nuclease free water + Optigene MM + gbpA LAMP primers + SYBR green; (Lane 6) gbpA + NEB MM + gbpA LAMP primers; (Lane 7) Nuclease free water + NEB MM + gbpA LAMP primers.
SYBR Green Optimization
SYBR Green was used to visualize amplification of miniprep DNA in the presence of UV light. 1 ul of SYBR Green was added to 25 ul of LAMP reactants (using NEB Master Mix, designed primers, & miniprep DNA for positive controls and water for negative controls). The samples were visualized at different wavelengths of UV light to determine the optimal wavelength for visualization and to optimize the concentration of SYBR Green in 25 ul of LAMP reactants.
Figure 5. Visualization of SYBR green at 302 nm and 365 nm for lmo0733 LAMP reaction.
No fluorescence was detected in the absence of SYBR green. Background fluorescence was observed in the negative controls. A clear distinction was observed between positive and negative controls.
Figure 6. Visualization of SYBR green at 302 nm and 365 nm for invA LAMP reaction
Results obtained matched the experiment performed with lmo0733. 1000X SYBR Green was determined to be the optimal concentration and 365 nm seemed to produce the best images for visualization of LAMP amplification.
SYBR Green Visualization
SYBR Green (1000X) was used to visualize the results of the LAMP reaction as determined by the optimization process detailed above. The gbpA gene was amplified using the LAMP method and fluorescence was detected in the positive sample at UV 254 nm as well as under blue light. The negative control showed background fluorescence, possibly due to the addition of primers or as a result of the SYBR Green itself. However, a clear distinction in fluorescence was observed.
Figure 7. Visualization of gbpA LAMP reaction with SYBR Green under UV (254 nm) and Blue Light
Colorimetric Visualization
NEB WarmStart Colorimetric Master Mix was used as a colorimetric dye to detect color change under visual light when the samples were amplified using the LAMP technique. The originally pink colored mixture turned yellow as a result of the amplification.
Figure 8. Colorimetric results from WarmStart Colorimetric Master Mix reactions with invA gene.
Colorimetric Test: Real Sample Swab and Amplification
To test the working principles of the Pathogene pathogen project, it had to be established that the intra-lab amplification techniques would be effective on real world samples of contaminated food, water, surfaces etc. Two samples of beef were prepared for the purposes of determining the colorimetric visualization of results for LAMP, in particular the use of NEB WarmStart Colorimetric Mastermix. A sample of untreated store-bought beef was prepared alongside a sample of DH5-alpha cells transformed with the lmo0733 gene from Listeria Monocytogenes. Direct swabs were taken from each sample and used in the LAMP reactions. Reactions lacking the target gene appear a bright red colour whereas reaction mixes containing the amplified gene appear salmon to yellow in colour.
Figure 9. Colorimetric results from WarmStart Colorimetric Master Mix reactions immediately after extraction from thermal cycler.
Figure 10. Colorimetric results from WarmStart Colorimetric Master Mix reactions 15 minutes after extraction from thermal cycler.
Figure 11. Agarose gel (1%) (left to right) : (a) 500bp ladder, WarmStart reaction mix with treated beef sample, WarmStart reaction mix with untreated beef sample, WarmStart reaction mix with nuclease-free water (b) 500bp ladder, Optigene reaction mix with treated beef sample, Optigene reaction mix with untreated beef sample, Optigene reaction mix with nuclease free water.
Both the visual colorimetric results immediately following and 15 minutes after the reaction show the treated sample of beef as having a distinctly lighter colour than the other two unamplified samples. The gel electrophoresis confirms the amplification of the lmo0733 gene from the whole swabbed bacterial cells and no amplification in samples without the target gene, assuring LAMP’s specificity.
LAMP Sensitivity (lmo0773, invA and hipO)
In order to determine the LAMP reaction sensitivity, the reaction was run with serial dilutions of miniprepped plasmid with the gene of interest. The reactions were set up according to Optigene or NEB LAMP kit protocols.
Figure 12. Agarose gel (1%) corresponding to the LAMP reaction with serial dilutions of miniprepped lmo0773, invA and hipO DNA. (a). lmo0773 serial dilutions 363 ng/µl, 200 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl. (b). invA serial diltioons 295.5 ng/µl, 200 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl. (c). hipO serial dilutions 172.5 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl
The sensitivity test corroborated that LAMP is a sensitive technique that can detect the DNA up to very small concentrations. Results obtained show that lmo0773 and hipO plasmids are sensitive up to 0.1 ng/µl, while invA plasmid is sensitive up to 0.5 ng/µl. Visually the amplification is comparably visible for all concentrations for lmo0773 and hipO plasmids, with miniprepped plasmid band being visible up to 25 ng/µl for all plasmids. The invA plasmid seems to not be as sensitive, however, as the literature reports LAMP to be sensitive up to 33 ng/µl, it is very likely that the invA plasmid is an outlier (6). The sensitivity of invA plasmid could have been affected by the improper set up of the reaction e.g. inaccurate serial dilutions, mistakes in the protocol, etc. Therefore, the test showed that LAMP is a good alternative technique, which is comparably sensitive to PCR.
In order to determine if visualization will be possible with the SYBR Green fluorescent dye even at low DNA concentrations, a LAMP reaction was run with hipO plasmid serial dilutions with 1 µl of 1000x SYBR Green dye added into the 25 µl LAMP reaction. Additional negative controls were included, such as SYBR Green + water and SYBR Green, water + hipO primers to determine the background fluorescence.
Figure 13. The SYBR Green fluorescence of the hipO serial dilutions represented under (a) UV light (365 nm) (b) Blue light (c) under Blue light with overexposure demonstrates.
The fluorescence results under UV and Blue light confirmed that the reaction can be visualized up to 0.1 ng/µl. Under UV light you can clearly see the difference between positive and negative controls. There is also a trend of decreasing fluorescence with decreasing plasmid concentration with the highest fluorescence at 172.5 ng/µl and lowest at 0.1 ng/µl. This is corroborated by the reaction vessels under the Blue light, which show the same trend. The overexposure option of visualization under the Blue light allows to show that even at 0.1 ng/µl there is more fluorescence than the background fluorescence present in the negative controls. Therefore, this test shows that even at low concentrations the SYBR Green is effective at showing the successful DNA amplification.
LAMP Specificity (lmo0773, invA and gbpA)
The same two experiments done with PCR were done with LAMP. The results obtained indicate that LAMP is highly specific as every gene was only amplified by its primers and not by any other primers. LAMP was found to be the only completely specific technique out of PCR, LAMP and RPA.
Figure 14. Agarose gels (1%) corresponding to LAMP specificity reactions carried out on two different genes lmo0733 and invA. The first set of reactions for each genes, (a) for lmo0733 and (c) for invA is done by keeping the gene constant while varying the primers, while the second set of reactions, (b) for lmo0733 and (d) for invA are carried out by varying the gene used while keeping the primers constant.
RPA
Reaction Volume Optimization
The original TwistDx RPA Basic kit protocol that is specified for a total reaction volume of 50 ul was optimized for the volumes of 25 ul and 10 ul. The amounts of reagents in the protocol stated for 50 ul were brought down proportionally and the reactions genes were amplified successfully as shown in the agarose gel (3%) images. The reactions were run with miniprepped plasmid with the gene of interest. Optimization of RPA reactions to lower volumes helped save RPA reagents in the experiments as well as in the microfluidic chips used for the amplification of pathogens in the Pathogene device.
Reaction volume: 50 uL reaction
Figure 15. Agarose gel (3%) showing RPA amplification of lmo0733, invA and gbpA miniprep DNA and transformed E. coli colonies in 50 ul volume reactions. The light bands seen in the negative control lanes are primer dimers and proteins from the RPA reaction. (Lane 1) 100 bp ladder; (Lane 2) lmo0733 miniprep + lmo0733 RPA primers; (Lane 3) lmo0733 transformed E. coli colony + lmo0733 RPA primers; (Lane 4) lmo0733 negative control; (Lane 5) invA miniprep + invA RPA primers; (Lane 6) invA transformed E. coli colony + invA RPA primers; (Lane 7) invA negative control; (Lane 8) gbpA miniprep + gbpA RPA primers; (Lane 9) gbpA transformed E. coli colony + gbpA RPA primers; (Lane 10) gbpA negative control; (Lane 11) 500 bp ladder
RPA reactions worked successfully for 50 ul reactions. To save lab reagents in experiments and to make the microfluidic chips economical in terms of resources, further experiments were carried out to test RPA reactions at lower volumes, i.e. 25 ul and 10 ul.
Reaction volume: 25 uL reaction
Figure 16. Agarose gel (3%) showing RPA amplification of invA and gbpA miniprep DNA and negative controls in 25 ul volume reactions. The light bands seen in the negative control lanes are primer dimers and proteins from the RPA reaction. (Lane 1) 100 bp ladder; (Lane 2) invA miniprep + invA RPA primers; (Lane 3) invA negative control; (Lane 4) gbpA miniprep + gbpA RPA primers; (Lane 5) gbpA negative control.
The reaction volume for RPA was successfully optimized to a total volume of 25 ul. This allowed for economical use of reagents in lab experiments and for use in microfluidic chips.
Reaction volume: 10 uL reaction
Figure 17. Agarose gel (3%) showing RPA amplification of gbpA, invA, and lmo0733 miniprep DNA and negative controls in 10 µl volume reactions. The light bands seen in the negative control lanes are primer dimers and proteins from the RPA reaction. (Lane 1) 100 bp ladder; (Lane 2) gbpA miniprep + gbpA RPA primers; (Lane 3) invA miniprep + invA RPA primers; (Lane 4) lmo0733 miniprep + lmo0733 RPA primers; (Lane 5) gbpA negative control; (Lane 6) invA negative control; (Lane 7) lmo0733 negative control.
The reaction volume for RPA was successfully optimized to a total volume of 10 µl. The agarose gel (3%) shows brighter bands for gbpA and lmo0733 compared to invA. This allowed for economical use of reagents in lab experiments and for use in microfluidic chips.
SYBR Green Optimization
SYBR Green was used to visualize amplification of miniprep DNA in the presence of UV light. 1 ul of SYBR Green was added to 25 ul of RPA reactants. The samples were visualized at different wavelengths of UV light to determine the optimal wavelength for visualization and to optimize the concentration of SYBR Green in 25 ul of RPA reactants, as was performed for LAMP.
Figure 18. Visualization of SYBR green at 302 nm and 365 nm for invA RPA reaction
No fluorescence was detected in the absence of SYBR green. Minimal background fluorescence was observed in the negative controls. A clear distinction was observed between positive and negative controls. 1000X SYBR Green was determined to be the optimal concentration and 365 nm seemed to produce the best images for visualization of LAMP amplification.
SYBR Green Colorimetric and SYBR Green Fluorescence Visualization for RPA
SYBR Green was used as the colorimetric and fluorescent dye to visualize amplified DNA from RPA. A color change from dark yellow to yellowish green is observed in the presence of DNA when SYBR Green (1000X) is added to the reaction mixture. Fluorescence is also detected at 254 nm.
Figure 19. (a) Visualization of SYBR Green color difference between positive and negative tests for the amplification of gbpA gene with RPA under visible light (b) Visualization of SYBR Green fluorescence difference between positive and negative tests for the amplification of gbpA gene with RPA under 254 nm UV light.
Background fluorescence was observed in the negative controls. However, a clear distinction was observed between positive and negative controls.
Figure 20. Visualization of SYBR Green fluorescence difference between positive and negative tests for the amplification of gbpA gene with RPA under 400 nm portable UV LED bulb.
Background fluorescence was observed in the negative controls. A clear distinction was observed between positive and negative controls.
Sensitivity for lmo0773 and hipO
To determine the sensitivity of RPA, the reaction was run with serial dilutions of miniprepped plasmid with the gene of interest. The reactions were set up according to the TwistDx RPA Basic kit protocol and it was optimized to reduce the reaction volume as mentioned earlier.
Figure 21. Gel corresponding to the RPA reaction with serial dilutions of miniprepped lmo0773, invA and hipO DNA. (a) lmo0773 serial dilutions 363 ng/µl, 200 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl. (b) hipO serial dilutions 159.8 ng/µl, 100 ng/µl, 50 ng/µl, 25 ng/µl, 10 ng/µl, 1 ng/µl, 0.5 ng/µl, 0.1 ng/µl.
The results obtained show that RPA is sensitive up to 0.1 ng/µl for both lmo0773 and hipO plasmids. Visually both plasmids have a clear amplification band that is comparable at all concentrations. The negative controls do not contain the specific amplicon band for either of the plasmids. The hipO plasmid has a smear at lower weight boundaries, however, it can be explained by the primer dimerization. Therefore, the test showed that RPA is an alternative technique that is comparably sensitive to PCR and LAMP.
Specificity
The two specificity experiments were done with RPA for the two genes, lmo0733 and invA. The results shown in the Figure below, show that RPA is not as specific as LAMP as amplification of a gene with primers designed for another gene does occur. This could be due to the fact that RPA uses the longest primers out of all three techniques, resulting in a higher possibility of having regions of the primers complementary to different genes.
Figure 22. Agarose gels (1%) corresponding to RPA specificity reactions carried out on two different genes (a) lmo0733 and (b) hipO. The first set of reactions for each gene is done by keeping the gene constant while varying the primers, while the second set of reactions are carried out by varying the gene used while keeping the primers constant.
References:
1. Nliwasa M, et al. (2016) The Sensitivity and Specificity of Loop-Mediated Isothermal Amplification (LAMP) Assay for Tuberculosis Diagnosis in Adults with Chronic Cough in Malawi. PloS one 11(5):e0155101.
2. Sarkar G, Kapelner S, & Sommer SS (1990) Formamide can dramatically improve the specificity of PCR. Nucleic Acids Research 18(24):7465.
3. Daher RK, Stewart G, Boissinot M, Boudreau DK, & Bergeron MG (2015) Influence of sequence mismatches on the specificity of recombinase polymerase amplification technology. Molecular and Cellular Probes 29(2):116-121.
4. Duan Y, Ge C, Zhang X, Wang J, & Zhou M (2014) A rapid detection method for the plant pathogen Sclerotinia sclerotiorum based on loop-mediated isothermal amplification (LAMP). Australasian Plant Pathology 43(1):61-66.
5. Duan .Kong X, et al. (2016) Development and application of loop-mediated isothermal amplification (LAMP) for detection of Plasmopara viticola. Scientific reports 6:28935.
6. Kong X, et al. (2016) Development and application of loop-mediated isothermal amplification (LAMP) for detection of Plasmopara viticola. Scientific reports 6:28935.
Here will go engineering stuff
A proper proof of concept is essential for communicating the breakthroughs in research and the property creation of a working device. As such, before building the device and integrating engineering and biology, each biological reaction was tested and the engineering working principles were verified and documented. More details on the process and tests themselves may be found in the biology and the engineering lab notebooks.
When a sterile cotton bud is used to collect a real life sample, amplification of the target gene and thus presence of the subject pathogen can be colorimetrically visualised in normal light conditions. Immediately after the LAMP reaction with WarmStart Colorimetric Mastermix is completed, there is a notably lighter appearance to the reaction tube containing the transformed bacteria with the target gene (lmo0733). On the other hand, the sample of uncontaminated beef and the negative control remain a bright red colour, the difference is more noticeable 15 minutes after the reaction. The gel electrophoresis confirms the amplification that occured. This set of experiments provides evidence that LAMP results can be visualised on real food samples with bacterial cells and not only on purified DNA samples.
Figure 1. Colorimetric results from WarmStart Colorimetric Master Mix reactions immediately after extraction from thermal cycler
Figure 2. Colorimetric results from WarmStart Colorimetric Master Mix reactions 15 minutes after extraction from thermal cycler
Figure 3. 1% agarose gel (left to right) : (left) 500bp ladder, WarmStart reaction mix with treated beef sample, WarmStart reaction mix with untreated beef sample, WarmStart reaction mix with nuclease free water (right)500bp ladder, Optigene reaction mix with treated beef sample, Optigene reaction mix with untreated beef sample, Optigene reaction mix with nuclease free water
Figure 4. Testing effective collection (using a swab) and release (passing water pressure through the swab) of a sample. Working principle appeared successful
Figure 5. Testing TE buffer chamber cross contamination from a contaminated used cotton swab. Small blue dots inside the chamber show cross contamination
Figure 6. Test the safe storage and effective release of the TE buffer using a film sealed plastic chamber released by a plunger
Figure 7. Testing flow of liquid in the first PDMS chip
The film was tested if it was hydrophilic enough to ensure good flow of liquid. When roughly testing wells and channels made only from the chip, it showed that the film is hydrophilic enough for liquid to flow without pressure.
Figure 8. Testing flow of liquid in the 3M chip
Confirming the hydrophilicity of the chip, a prototype made from double sided tape and film was tested. The chip had a channel width of 200µ m, which is a conventional width for PDMS microfluidic chip. However, the liquid did not flow to the wells. Through varying different width of the microfluidic chip, we realized that maximizing the surface area exposed to the hydrophilic film is more important than varying surface pressure of the wells. The finalized chip had a 600µm width to ensure good flow but prevent flowback.
The reagents for two positive as well as two negative NEB LAMP reactions were added to four different wells on PDMS chip. Each reaction contained 12.5µ l of mastermix, 9 µ l of water and 1µ l of miniprep DNA. Positive control reactions contained 2.5µ l of primers, while in negative control reactions, the same volume of water was added instead. After the reagents were added to the chip, it was covered with hydrophobic PCR tape in order to prevent evaporation of the reagents throughout the reactions.The reactions were then run for 30 minutes by placing the chip on a hot plate heated to a temperature of 65°C. Figure 1 shows the chip as viewed under blue light. The wells containing positive are marked with a + symbol while the negative controls are marked with a - symbol.
Figure 9. Positive and 2 negative LAMP NEB reactions run in a PDMS chip
Next, the four RPA reactions were carried out in a 3M chip. For one RPA reaction, 29.5 µ l of re-hydration buffer was added to one tube of dried reaction, along with 2.4µ l forward primers, 2,4 µ l backward primers, 8.2µ l of water, 5µ l of DNA, 1µ l of 1000X SBYR Green and 2.5 µ l of Magnesium acetate. The primers were replaced with an equal volume of water for the two negative control reactions.
Figure 10. Positive and 2 negative RPA reactions run in a 3M chip
The heating device provides a platform that sustains the designated temperature under which the RPA, LAMP reaction should run. There are three modes for the device: in the first mode, the green LED light lights up, signaling that the power is connected. The 6 blue LED lights that aids visualization will also be on. In the second mode (for RPA reaction), one red LED light turns on, and the heating board heats up to and maintains at approximately 40°C. In the third mode (for LAMP reaction), two red LED lights turn on and the heating board heats up to and maintains at approximately 65°C. A temperature sensor is closely attached to the heating board and helps ensure that the temperature is maintained as desired.
Figure 11. The second mode of the circuit that heats up to and maintains at about 40°C
Figure 12. The third mode of the circuit that heats up to and maintains at about 65°C
Ten NEB LAMP reactions were run, five of which were positive controls with both DNA and primers added, while the other five were negative with DNA added but with no primers. The reactions were run in PCR tubes at 65°C for 30 minutes. The completed reactions were then pipetted into the wells of a ten-well PDMS chip, alternating between positive and negative.
The objective of this was to ensure that fluorescence could be observed in the PDMS chip under blue light. Moreover, this was done to illustrate the difference in fluorescence between positive and negative controls.
In the chip below shown in Figure 13, the difference in fluorescence, as viewed under blue light, between the positive and the negative samples is clear.
Figure 13. Five positive and five negative LAMP NEB reactions, run in PCR tubes and pipetted into a PDMS chip
The same process was repeated using 3M chips. 10 reactions, 5 positive and 5 negative were carried out in PCR tubes and pipetted into a 3M chip to check visualization. The results are shown in Figure shown below, as visualized under blue light.
Figure 14. Five positive and five negative LAMP NEB reactions, run in PCR tubes and pipetted into a 3M chip to check visualization
