|
Using an inducible hybrid light-sensitive promoter for heterologous
regulation of the nif cluster
Benjamin Huang, Jeffrey Lee
Synthetic biology is an exciting area of research that aims to
genetically improve organisms to make them more efficient and hopefully
more useful to us as well. The human population in 1950 was 2.5
billion, yet it is predicted to surpass 9 billion by 2050 [1]. Even
with population growth slowing, increasing life spans and standards of
living will soon tax our natural resources. One of the most concerning
is our food supply. The agriculture industry needs a revolution in
order to keep up with our expected growth rates. Currently about 80% of
chemically fixated nitrogen is used as agricultural fertilizers, the
majority in developed lands [1]. Intracellular nitrogen fixation in
crops could help to sustain the burgeoning world population, especially
in areas with less fertile soil without taxing the planet’s waterways.
The exponential increase in nitrogen fertilizer has led to more runoff
into rivers and oceans. Fertilizers then provide nutrition for algal
blooms that result in hypoxia and form oceanic dead zones. These dead
zones lead to the death of marine species and have potentially large
economic consequences.
The ramifications of nitrogen fertilizer runoff can be averted by
genetically engineering plant crops to fix their own nitrogen. Some
cyanobacteria fix nitrogen for nutritional needs, while most organisms
can only acquire it from the food it consumes. Synthetic biology allows
us to transfer this ability to fix nitrogen to a heterologous host that
has many genetic tools, Escherichia
coli, so that we can learn how to give single cell organisms,
and eventually chloroplasts the ability to create their own nitrogen
fertilizer.
Diazotrophic (organisms that fix nitrogen) cyanobacteria such Nostoc
Punctiforme or Anabaena
use heterocysts (specialized nitrogen fixing
cells) to create a mini-anaerobic environment to aid nitrogen fixation.
However, Cyanothece 51142, a
non-heterocyst, fixes nitrogen in the same
cell as photosynthesis by relying on a circadian metabolic process,
when there is less oxygen byproduct from photosynthesis. Our goal this
summer is to engineer the regulation of the proteins necessary for
nitrogen fixation so that they are highly repressed when activated by
broad spectrum light (such as the sun), and are highly active when
there is no light around, mimicking the cycle where photosynthesis
occurs during the day and nitrogen fixation occurs at night.
Traditionally, gene expression has been induced through chemical means.
However, this method requires expensive chemicals, and can have
deleterious side effects on cell health. In Tabor et. al (2010), it was
shown that it is possible to induce expression of a reporter gene with
light in E. coli using light
sensitive proteins (CcaR/CcaS) from the
model cyanobacterium Synechocystis
S. 6803. Light induction has several
advantages over chemical induction, including: long term cost of
chemical inducers, ability to tune expression levels with different
light intensities, and most importantly, can be turned on and off
easily. The ability to control genes of interest has important
applications in engineering nitrogen fixation. The end goal of our
project is for plants to fix nitrogen on their own within their
chloroplasts--the true powerhouse of plant cells, where the most ATP is
present to overcome the high costs associated with breaking nitrogen’s
triple bond.
Objectives
Synechtocystis PCC6803
(hereafter S. 6803) is a strain of cyanobacteria that is of particular
interest to us. S. 6803 is important because it is the first
cyanobacteria to have its complete genome sequenced; and it is easily
manipulated via homologous recombination. Another aspect of S. 6803
that renders it a relevant is based on the ultimate goal of allowing
plants to fix their own nitrogen. Nitrogen fixation in these
genetically engineered plants would have their own cellular machinery
(analogous to chloroplasts and mitochondria) that direct the evolution
of nitrogen. Based on the Endosymbiotic theory, chloroplasts and
mitochondria are thought to have been cyanobacteria that were engulfed
by cells. Thus, S. 6803 is an important platform from which further
manipulation of the nitrogen fixation can occur.
Recently it has been shown that one can induce via green light, the
expression of a phycobilisome-related gene [2]. Instead of regulating
gene expression via proteins, having to worry about different
concentration levels, potential cross effects, etc., regulation via
light can be easily tested for and manipulated as well. Therefore, we
propose to design a hybrid inducible light-sensitive promoter for
heterologous regulation of the nif cluster in E. Coli.
Approach
We created a 4 piece assembly plasmid integrating light regulation
components from pJT122, but swapping out cph8 (for EYFP from pSL2264)
and lacZ (for TetR from pTet-PP*) and combined them into a plasmid
PBJ003 which should repress expression of EYFP when induced by light.
PBJ003 is controlled by the basic cpcG2 promoter driving TetR
production. We also created a hybrid promoter to swap out for the basic
cpcG2 promoter. Both these parts are on the registry under BBa_K1385000 and BBa_K1385001.
 |
 |
Hybrid promoters that integrate the regulatory elements from several
sources have been shown to be functional with varying levels of success
[3]. Operator sites for the green-light sensitive PcpcG2 promoter are
well known [4], additionally, the hybrid trc1O promoter has been shown
to be highly expressed in E. coli (22-fold induction) even without IPTG
[5]. The trc1O promoter has one lac operator site and is thus easier to
induce than the more tightly repressed trc2O that contains two
repressor binding operator sites.
In order for PcpcG2 to function as a light-sensitive promoter, a
histidine kinase CcaS and response regulator CcaR will be required.
Upon exposure to green light, CcaS is auto-phosphorylated and then
phosphorylates CcaR. This changes the DNA binding affinity to CcaR
allowing CcaR to bind to PcpcG2 and activate transcription. This could
be obtained by creating our own plasmids with these genes (already
done). Our hybrid promoter could be cloned into a vector that contains
a fluorescent reporter protein EYFP driven by EYFP to compare the
strength of transcription when activated by light in E. coli containing
both CcaS/R, eventually allowing the light promoter to regulate the nif
cluster. |
|
 |
A few
factors have been taken into consideration for the design of the
hybrid promoters. The consensus sequence known as the “G-box”, a highly
conserved direct-repeat motif located 109 and 108 bases upstream of the
transcription start site in N. Punctiforme and S. 6803, is a region
where CcaR binds to PcpcG2 as an activator [4]. We choose to use Ptrc1O
and keep the whole sequence intact because it is shown to be highly
repressible and easily inducible and thus should essentially work as a
constitutive promoter in E. coli, even though it has been reported to
be leaky in S. 6803 [5]. By combining the upstream components (CcaR
binding site) of PcpcG2 with Ptrc1O, while keeping the Ptrc1O ribosomal
binding sequence intact, our hybrid PcpcG2/trc1O promoter in E.
Coli
should be highly expressed in (green) light with basal levels of
transcription without lig |
|
As described above, the hybrid
promoter functions the opposite of how
we eventually want it to; namely, we want nitrogenase to be highly
repressed in light conditions (where a lot of oxygen will be present to
poison nitrogenase), and highly expressed in the dark. Therefore we
need to create a genetic switch that functions essentially as a NOT
gate, where in high light conditions, our product (currently EYFP),
will be highly repressed.
Different switches based on RNA have been well documented in E. coli;
we have several options. First we are testing the repression mechanism
using a basic pTet/TetR, repression mechanism. By expressing TetR, the
system driven by the hybrid promoter should show strong repression in
light, and strong expression in dark.
Our next step would have been to swap out the pTet/TetR repression with
a system of CRISPR interference to block transcription initiation or
elongation based on binding to the template or non-template strand of a
chosen sequence [9]. In our case, we would tune the sgRNA to bind to
the -35 box of our hybrid promoter in order to block transcription. The
reason we want to use CRISPRi is because it has been shown to be
functional in both prokaryotes and eukaryotes, although slightly more
complex, this becomes a much more powerful tool once people transition
to eukaryotic environments. Both of these genetic switches should be
able to highly repress our fluorescent protein when induced with light.
Meanwhile, once the other half of our iGem team gets nif cluster
working in E. coli, we should be able to swap out the fluorescent
protein for the nif cluster in our plasmid to regulate the nif cluster
in E. Coli with light. In dark conditions, the switch will be “off”,
namely there should be fluorescence; and in the light, the system
should be repressed. We expect to see higher levels of repression with
our hybrid promoter and greater dynamic fold change.
|
 |
| Our project
goals are to design a hybrid promoter that incorporate the
regulatory elements of PcpcG2 with those of Ptrc1O. Then we will
transition to the more complex CRISPRi mechanism by creating a plasmid
containing the basic trc1O promoter that reversibly blocks
transcription of EYFP. The overarching plan is to be able to regulate
the nif cluster with light, so nitrogenase is only expressed during the
dark, which mimics Cyanothece
51142. If successful, this project would help immensely when eventually
integrating nitrogen fixation into plants by improving efficiency.
During the day, when photosynthesis occurs (with a lot of oxygen as
byproduct) nitrogenase would not be produced, and therefore not wasted;
while during the night, nitrogen fixation can occur. This creates a
temporal regulatory system orthogonal to Cyanothece 51142’s native
circadian regulation of controlling nitrogen fixation (through
metabolic pathways), increasing the overall chance of success. |
Condition
|
Product
|
Fluorescence
|
Light
|
TetR
|
Basal
|
Hybrid
Light
|
TetR
|
None
|
Dark
|
EYFP
|
High
|
|
 |
By
integrating the light regulation from S. 6803 into E. coli, we are
transitioning to the next step in our big picture, which would be to
get the system working in the cyanobacteria S. 6803. Eventually we want
our system to be able to work in chloroplasts of plants, so nitrogen
fixation will be able to occur in the same location where the most
energy is produced without having to worry so much about the oxygen
byproduct of photosynthesis. |
Summer PROPOSED
Work Flow
Week 1: Familiarize self with standard laboratory methods and
procedures. Design primers for transcriptional units and plasmid
backbone.
Week 2-3: Test light regulation in pBJ003 (driven by basic PcpcG2). Use
positive and negative controls as well to ensure system is working as
intended with EYFP fluorescence as our gene expression.
Week 4-5: Swap out basic PcpcG2 in pBJ003 with our hybrid promoter and
test for increased Fluorescence of EYFP.
Week 6-8: Swap out tetR/ptet with CRISPRi mechanism with dCas9 and
sgRNA plasmids. If things go as planned, swap out EYFP with nif cluster
in hybrid promoter driven plasmid.
Week 9-10: Analyze data, comparing fluorescence in different
intensities of light, wavelengths, time intervals, etc.
Our general workflow for each plasmid cloning is as follows:
a. Primer design for backbone and pieces
b. PCR pieces for amplification
c. Run a gel extraction
d. Gel DNA Recovery
Treat with DpnI and purify if necessary
e. Digestion/Ligation (Golden Gate or Blunt End)
f. Transformation (Electroporation)
g. Plate and grow overnight
h. Pick colonies and start liquid culture overnight
i. Freeze and Miniprep cultures
j. Run sequencing PCR to check junctions
k. Run visualization gel for sequencing PCR
l. Send for sequencing
m. Verify sequence products are as intended
With every step there is a chance that things could go wrong, and we
would troubleshoot in order to determine the best course of action
going forward.
Data
Figure above: Original Light induction experiment once all the cloning
was over. No fluorescence seen.
After all our cloning mishaps
we finally were able to test our light induction system. However,
nothing worked as expected. The data represented above is the
fluorescence normalized to the absorbance, or OD of the strains we
grew. We essentially had the same fluorescence as our negative control,
and even when we induced with 250ng/mL of ATC we saw no fluorescence.
This led us to run a few more experiments to troubleshoot the plasmids.
|
 Figure
above: We ran another crude experiment to check what could be the issue.
Our original positive control
was under control of constitutive promoter, J23100, and was the only
thing we got to fluoresce. We were concerned with competing translation
start sites so we cloned a plasmid that modified the RBS to allow for
EYFP to fold properly, but fluorescence only got weaker. We then
decided to swap out the pTet promoter and lo- and behold got
fluorescence. Our next step was to swap out the reporter mechanism of
our experimental plasmids.
|
Figure above: Fluorescence in
the dark (when promoter not active) same regardless of chromophore
presence.
|
|
Results
Figure above: Final Light
experimental data
|
Normalized fluorescence is compared to the positive control after
subtracting the negative fluorescence value. The Hybrid 0 aTc results
in light ended up fluorescing even less than the negative control,
implying the system is completely off, which is what we ideally want.
Another thing to note is that the system isnt working 100% as expected,
but it is still promising.
When comparing light to dark values, the general trend is there, but
the repressor is very leaky. There is so much tetR in around that it is
dominating the system; with no aTc around, there is so little
fluorescence, but once we add a meaningful amount of aTc, we are able
to see results closer to what we expected. In the dark, we want our
fluorescence to be relatively high, comparritive to the positive
control, and we want the system to be highly repressed in the light
(without having to induce with aTc).
When we compare the hybrid promoter to the normal cpcG2 promoter, it
seems like there is a bigger change between dark and light in the
system. In constant light, aTc is known to degrade, which is why some
of the fluorescence might still be there. Hence, in the light we do not
know how much of the repression is due to the strength of the promoter,
or the reduction of aTc. It is apparent that the hybrid promoter is
leakier than the original- even with a high concentration of aTc we see
very little fluorescence in the light. A comparable amount of aTc would
have degraded in the light of both the hybrid and normal promoter, but
it is hard to say if the difference in both light values with aTc would
have been as apparent without the degradation of aTc.
Our next steps would be to modify the RBS of TetR in order to find a
saturation point where the system is most tightly on and off without
aTc. We ideally do not want to use aTc at all, as chemical induction is
troublesome and won't be very reliable if degraded by constant light.
After we modified the system to be working without aTc around, we can
look into swapping EYFP with the nif
cluster to have the genes expressed only in the dark.
|
1. Rogers, Oldroyd. Journal of Experimental Botany March 2014
doi:10.1093/jxb/eru098
2. Hirose, Shimada, et al. PNAS July 15, 2008 vol. 105 no.28
3. Lutz and Bujard Nucleic Acids Research, 1997, Vol. 25, No. 6
4. Hirose, Narikawa, et al. PNAS May 11, 2010 vol. 107 no. 19
5. Huang et al. Nucleic Acids Research, 2010 Vol. 38 No. 8
6. Tabor, Levskaya, et al. J. Mol. Biol. (2011) 405, 315-324
7. Kim, White, et al. Molecular Systems Biology 2006
doi:10.1038/msb4100099
8. Brantl, Wagner. J. Bacteriol. 2002,
doi:10.1128/JB.184.10.2740-2747.2002.
9. Larson , Gilbert, et al. Nature, Oct. 2013 vol. 8 no. 11
10. Abe, Koichi, et al. Microbial biotechnology (2014).
|
"
