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In this section, we will explain the
In this section, we will explain the design of our DNA Shell .
==Main structure of DNA shell==
==Main structure of DNA shell==
Revision as of 00:50, 28 October 2012
In this section, we will explain the design of our DNA Shell in detail.
Main structure of DNA shell
Our DNA Shell is designed as DNA Origami. In this section, we explain about DNA Origami, and then describe about our design of the typical structure and added functions of DNA Shell. Also, we simulated about stability of hybridization.
DNA Origami is a complex 2D or 3D structure which is fabricated using herical structure of DNA. Generally, DNA Origami is composed of one Scaffold DNA, long single strand DNA, and many Staple DNA, short single strand DNA. Staple sticks a part of scaffold to the other part and achives the designed structure. For designing DNA Origami, the phase of hydrogen bond of DNA herical structure should be concerned. We could easily design DNA Shell using CADNano®, the software for designing DNA Origami.
For our DNA shell, we used a typical DNA material called M13 as scaffold DNA. It has approximately 7250 base pairs and it is an ideal number for our shell. Some parts of this DNA hybridizes by itself, so we had to cut those parts off for our further design. In designing the staple DNAs, we standardized the number of base pairs to 32 bp, because the characteristic of hybridization is greatly affected by the number of base pairs.
Fig. 1.1 is the picture of DNA Shell on CAD Nano. The blue line is scaffold and the others are staples. the shell has three large domains which are about 40nm × 30nm. the center and right domains are the body of the shell and able to be added various functions. the left domain is used for immobilizing in microchannel. When hybridizing scaffold and staple, the tempereture in which the reaction is stable is determined by the length of staple, so we designed almost staples as same length. Furthermore, if the staples of the bridges which connect the domains are not added when hybridizing, these part of scaffold can be freely deformed, and shell can open and close like real shell.
In order to add functionality to the body, we extended some of the staples so they could bond with DNA fragments that are modified (Fig. 1.2). Therefore, we added 13 base pairs to the staples which originally had 32 base pairs. We designed all these staples to extend from the same side of shell surface taking care of the phase of the hydrogen bond.
We needed to attach 12 single-stranded DNAs with fluorescent molecules (named as fluorescent DNAs) and two functional single-stranded DNAs to one side, and 12 single-stranded DNAs with quenching molecules (named as quenching DNAs) and two functional single-stranded DNAs to the other side. We had to think up of 4 different sequences that would bind to either:
- fluorescent DNAs
- quenching DNAs
- functional DNAs to the fluorescent side
- functional DNAs to the quenching side
We designed the structure so that the functional part is surrounded by fluorescent/quenching molecules (Fig. 1.3). For working quenching molecules appropriately, we designed the fluorescent molecules and the quenching molecules to face each other.
Simulation techniques were applied in the design to make sure that the staples are hybridized only at the points where we want hybridization to occur. That is, we have to keep the energy for hybridization high in inappropriate areas and keep it low in the correct areas. In order to achieve this requirement, we focused on these three points.
- Make sure that the complementary arrangements of the designed staples does not appear in inappropriate area.
- Keep the melting temperature of correct hybridization low, and keep the melting temperature of incorrect hybridization high.
- Avoid steric hindrance.
The combination of Watson-Crick base pair is stable, therefore if there are no other possibilities of hybridization of the staple and the scaffold in inappropriate areas, the energy of hybridization would become the lowest in the appropriate area, which means that the possibility of achieving our first focus, correct hybridization will increase. Also, we achieved the second requirement through trial and error. If we hybridized the arrangements extended from staples and functionalized parts simultaniously, there would be some steric hindrance. To weaken this effect, we set a realm where the staples will not be hybridized. Concretely, we embedded two T (thymine) bases in the staples.
To simulate the energy of hybridization and melting temperature, we used the software named DINAMelt and NUPACK supported on online. Since there is no absolute solutions for design, we needed to get over the difficulties by trial and error; It was serious and troublesome work. In designing the arrangement extended from staples, we need to attach the same arrangement to the staples attached with functional parts. This work of discovering moderate arrangement cost us immense labor, because it is required to make these staples added only ONE pattern of arrangement hybridized stably. The work of discovering a arrangement compatible to several staples was like finding one penny lost somewhere in campus.
Fig. 1.4 is one example of simulation using DINAMelt (http://mfold.rna.albany.edu). This is a simulation of the melting temperature and the possibility of correct hybridization. This is simulated under a situation of
- From 0°C by 1°C to 100°C as DNA
- [A0] = 1.6e-07 M, [B0] = 1.6e-07 M ;[A0] is concentration of extended staple and [B0] is concentration of modified functional part
- [Na+] = 0.2 M, [Mg++] = 0.0125 M
As seen below, a hybridization of A and B (appropriate hybridization) is dominant at low temperature(from 0°C to 30°C).
In this section, we write about our experiment. Our experiment consists of four themes;
- Assembly of the DNA Shell
- Capturing Ability
- Immobilizing on microfluidic device
- Supporting enzyme
In each theme, we experimented this summer and can get various valuable data. we wrote our data and results in order.
Assembly of the DNA Shell
First, we mixed M13 and staples, and ascertained whether DNA Shell was hybridized as we had designed by agarose gel electrophoresis and atomic force microscope (AFM).
The staple DNA was mixed with M13 (160 or 16 nM of each staple DNA, 1.6 or 4 nM of M13, a 100 or 4 –fold excess of staple DNA) in 1x TAE/Mg buffer. When we added functional staples which are DNA with molecules such as the fluorescence, the quencher and the biotin instead of normal staples, we made the density of functional staples all the same as normal staples. Samples were annealed two hours from 95℃ to 20℃ in a thermal cycler at a rate of 6.25℃/10minutes 12 steps.
Agarose Gel Electrophoresis
We confirmed that we had the structure which had the bigger molecular weight than original M13(scaffold) by electrophoresis. Samples were electrophoresed in a 0.6 % agarose gel containing 1X TAE/Mg buffer. The agarose gel was run at 4℃ for 70 minutes (Fig.1 & 2).
The band of M13+staple ran longer than the band of M13. It showed that the structure which had big molecular weight was created. The lower fuzzy band was the band of excess staple DNA. When we put staples both 100 and 4 times of M13mp18, the annealing went well.
These DNA origami (M13 + all staples) were observed by using AFM to confirm that these DNA Shell were formed correctly. 1xTAE/Mg solution was utilized as buffer.
This AFM picture clearly shows that the origami with all staples was formed as designed. There was the point where it seemed that origami connected with each other aside. This is probably because each DNA Shell was attracted each other by π-π stacking interaction. We designed DNA Shell as base pair lined lengthways, so it was appropriate for DNA Shell to connect sideways by π-π stacking interaction.
Next, we ascertained whether DNA Shell captured target molecules (target DNA, streptavidin) by agarose gel electrophoresis, fluorometry, and AFM.
Agarose gel electrophoresis
We ascertained whether the migration distance changed after target DNA was added in the solution with DNA Shell. After having annealed the sample which added target DNA (control1 and control2) to M13 and staple, we electrophoresed and confirmed a change of the phoresis distance. Samples were electrophoresed in a 0.6 % agarose gel containing 1X TAE/Mg buffer at 4℃ for 70 minutes.
All the samples which were added target DNA to come to have a shorter phoresis distance than the sample which wasn’t add. It is thought that it became hard to go through the mesh of the gel by Shell having been closed.
After having annealed the sample which contained M13, staple DNA, DNA with a fluorescence molecule and DNA with quencher molecule, we took the sample 100μl and added 1xTAE/Mg buffer 400μl and measured the fluorescence intensity. We recorded a fluorescence change when we put target DNA.
Fluorescence change (1 equal amount of target DNA)
After having added target DNA, intensity of fluorescence decreased. It is thought that the fluorescence decreased because Shell closed by having put target DNA and fluorescence molecules approached quencher molecules.
The next graph is the change of the peak numerical value when we changed the density of target DNA. We calculated peak numerical value after having added target DNA for 100 at the intensity of fluorescence of the peak before adding target DNA.
We changed the number of fluorescence molecules and the quencher molecules which spread from the Shell surface (12, 4 or 1) and, in the case of each, checked how became a fluorescence change. In the lower graph, peak numerical value before adding target DNA is 100.
In the case of 12 and 4 fluorescence molecules, there is not the big difference, but there is a bigger fluorescence change than in case of 1 fluorescence molecule. It may be said that this becomes easy to detect a fluorescence change because plural fluorescence molecules approach with quencher molecules at a time when Shell was closed when density of target DNA is small.
Following target DNA, we checked whether we could capture streptavidin with Shell.
After having annealed the sample which contained M13, staple DNA, DNA with a fluorescence molecule, DNA with quencher molecule and DNA with biotin, we took the sample 100μl and added 1xTAE/Mg buffer 400μl and measured the fluorescence intensity. We recorded a fluorescence change when we put SA.
Fluorescence change (1 equal amount of SA)
After having added SA, intensity of fluorescence decreased. It is thought that the fluorescence decreased because Shell closed by having put SA and fluorescence molecules approached quencher molecules.
Changing the density of SA
The next graph is the change of the peak numerical value when we changed the density of SA. We calculated peak numerical value after having added SA for 100 at the intensity of fluorescence of the peak before adding SA.
A fluorescence change of 1/8 equal amount of SA is the biggest. It is thought that a fluorescence change becomes small, when SA density is big, the SA of 2 molecules is connected to biotin spread from two sides of Shell, and Shell does not close and when SA density is small, a ratio of Shell to close is small.
We performed fluorimetry in three kinds of Shell ( Shell where biotin grew on both sides (Normal Shell)  Shell where biotin grew only in the fluorescence side  Shell where biotin grew only in the quencher side).
There was not the big difference between  and . However, only  came to have a particularly big fluorescence change. The 2 molecules of biotin grow from one Shell in  and . Because 4 molecules of biotin are connected for 1 molecule of SA, it is thought that two Shell catched one SA, and a dimer was formed. In this case a large number of fluorescence molecules would approach at a time in , and it is thought that concentration quenching happened, and the fluorescence decreased.
First, we tried the version of target DNA. This picture was captured by AFM. In the picture, some square-like structures could be seen. They are exactly DNA Shell. And it is observed that almost central part of the Shell is white. This shows that central part is thicker than the other part of it.
We found that the thickness of the white point in the Shell (Fig.188.8.131.52) was about 4.9nm(Fig. 184.108.40.206). In this picture, the left upper graph shows the sectional pitch that cut Shell perpendicularly. Target DNA is 26bp or about 5.8 nm, so we estimate that target DNA hybridized with staple DNA with a little curve.
Following target DNA, we checked whether we could capture streptavidin with Shell. At the upper left of the above picture, we could see the square structure which has two white points in the center. This structure is the Shell. The following pictures show the sectional pitch.
These pictures show:
- Shell is 91.797nm (almost 90nm) width
- Shell is 2.075nm (almost 2nm) thick
- The white points of Shell are 3.882nm and 4.096nm(almost 4nm) thick
- There is a part with almost 0nm thick at around 21nm from the side of Shell
Shell is constructed from double helix, so it is reasonable to think that the value 2nm is Shell's thickness. The thickness at the white points in the Shell are equivalent to the thickness for approximately two folds of double helix. In addition, width of Shell at the design stage is approximately 120nm and the structure seen this time, width is almost 2/3. It is reasonable to suppose that this is because one outer sheet of the Shell is on top of the other sheet. That's why we estimated that Shell captured streptavidin. The white points of the Shell are small compared with the Shell itself because streptavidin is small (almost 60 Å)
Immobilizing on microfluidic device
We confirmed DNA origami is immobilized on the surface of microfluidic device.
Control is introduced into microfluidic device
- A solution containing of fluorescent labeled-DNA origami(M13 + staples) was introduced into a microchannel on the microfluidic device. After rinsing to remove DNA origami not immobilized on the microchannel, observation of fluorescence from immobilized DNA origami was performed (a). The scale bar is 100 μm.
- The fluorescence was almost kept even if water is introduced into the microchannel (b).
- The fluorescence strength would be weak when the control solution is introduced into the microchannel (c).
And we showed the fluorescence intensity of each image to the graph.
After water was introduced, decreasing of fluorescence intensity was observed due to destruction of immobilized DNA origami. Changes in salt concentration by introducing water makes it happen. Also after control was introduced, fluorescence intensity was greatly decreased. Fluorescence weakened greatly because the control was attached to the DNA origami immobilized on the microchannel.
Therefore, we confirm that DNA origami was immobilized onto the surface of the microchannel.
Streptavidin is introduced into microfluidic device
- A solution containing of fluorescent labeled-DNA origami(attached Biotin) was introduced into a microchannel on the microfluidic device. After rinsing to remove DNA origami not immobilized on the microchannel, observation of remaining fluorescence from immobilized DNA origami is performed (d). The scale bar is 100 μm.
- The fluorescence was kept when water is introduced into the microchannel (e).
- The fluorescence strength would be weak when the streptavidin is introduced into the microchannel (f).
And we showed the fluorescence intensity of each image to the graph.
Since number of times of rinsing was few, DNA origami which was not immobilized was not removed. So after water was introduced, fluorescence intensity greatly fell. Also fluorescence intensity became weak after the streptavidin was introduced. Fluorescence weakened because the streptavidin was attached to the DNA origami immobilized on the microchannel.
Based on the results mentioned above, we did further advanced experiments. We confirmed whether DNA Shell supported enzymes.
We used 3,5,3’,5’-tetramethylbenzidine (TMB), streptavidin with horseradish peroxidase (HRP) labeling and trypsin. TMB can be oxidized for the reduction of hydrogen peroxide (H2O2) to water by such as HRP.
We make use of two biochemical reactions;
(1) TMB is oxidized by H2O2/HRP. This reaction happens with a change of color. When TMB (λmax=285nm) is oxidized, the solution takes on a blue color (λ=370 and 652nm) at first and gradually turns to yellow (λmax=450nm). ( Josephy, P. D., Eling, T., and Mason, R. P.(1982) J.Biol.Chem, 257, 3669-3675)
(2) Trypsin, a protease that cleaves peptide chains mainly, decomposes HRP. (Welinder, K. G. (1979) Eur. J. Biochem, 96, 483-502)
If trypsin decomposes HRP, before the reaction happens between TMB and HRP, HRP does not oxidize TMB. Furthermore, we used streptavidin-labeld HRP and DNA Shell with biotin. DNA Shell protects HRP because of the combination between streptavidin and biotin. As HRP protected by Shell, trypsin does not decompose HRP and the oxidization of TMB goes on.
We made four kinds of solution like below (Table 2.4.2) and measured the absorption spectra of each solution.
|TMB||HRP||Trypsin||DNA Shell||Expected Peak Wavelength[nm]|
Table 2.5.2 Four kinds of solution for the experiments.
- (No.1) We only used 2μM TMB in acetate buffer.
- (No.2) We added 20nM streptavidin-labeled HRP in tris HCl to the solution of 2μM TMB in acetate buffer.
- (No.3) We added the solution in which we reacted trypsin and HRP for 1 hour in 37C constant temperature bath and HRP to TMB. As a whole solution, 0.2µM TMB, 2µMHRP, excess trypsin and 50mM acetate (TMB buffer), 50mM trisHCl (HRP buffer) are contained.
- (No.4) We added the solution in which we reacted trypsin, HRP and Shell for 1 hour in 37C constant temperature bath and HRP to TMB. 0.2µM TMB, 2µMHRP, 2nM DNA Shell, excess trypsin and 50mM acetate (TMB buffer), 50mM trisHCl (HRP buffer) are contained.
Results and Measurements
Please refer to below link.