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Revision as of 03:56, 22 October 2019
D E S I G N
Design
“Always plan ahead. It wasn’t raining when Noah build the ark” - Richard Cushing
What does expanding the golden gate based Marburg Collection, automating time consuming lab work and establishing the
CRISPR/Cpf1 system in Synechococcus elongatus UTEX 2973 have in common?
To achieve these objectives, it is always necessary to have a comprehensive theoretical preparation. It all starts with
literature research, summarizing the current state of the art and based on this developing own ideas. To have the theoretical
background settled before the lab work starts is a key point of every project and consumes many hours.
Because in the near future phototrophic organisms will get more and more relevance for biotechnological applications,
we want to establish the use of Synechococcus elongatus as a phototrophic organism for synthetic biology. Following the
principles of synthetic biology to simplify the process of engineering of biological systems, we set it our goal to establish
Synechococcus elongatus UTEX 2973 as the fastest and most accessible phototrophic chassis to date, providing it as a
wind tunnel for phototrophic organisms with user friendly and standardized workflows.
In order to achieve these goals, a lot of effort has been put into designing, building, testing, evaluating and learning.
Further, these steps had to be iterated over and over again to elaborate our standardized designs. By providing you our
theoretical background we want to give you an insight in our decision-making.
Strain Engineering
In Strain Engineering we modified Synechococcus elongatus UTEX 2973 to establish the CRISPR/Cpf1
system in our organism.
(Further we tailored strains that the organism suits to several experimental
setups and domesticated a wild type plasmid for further genetic manipulation.)
Strain Engineering
Natural Competence
As mentioned in our description, Synechococcus elongatus UTEX 2973 is no
longer
naturally
competent, presumably due to a point mutation in the pilN gene ( Li et al., 2018 ),
which means that when genetically engineering this organism other ways to introduce exogenous DNA have to be
taken into consideration. This is mainly done through electroporation or conjugation - especially
triparental conjugation (Yu et al., 2015) .
Triparental conjugation into the UTEX 2973 strain is typically performed with two E. coli HB101
strains, one
harboring the pRL443 and one harboring the pRL623 plasmid. The latter strain is then again transformed with
the
plasmid of interest, the prior is used as the conjugal strain - both have to be incubated together with the
cyanobacteria for the conjugation to take place (Wendt et al.,
2016)
To overcome this time-consuming process, we planned to reintroduce natural competence into our strain.
It
was already shown, that this can be done by integrating an intact copy of the pilN gene into one
of
the
neutral sites
(Li et al., 2018) , though this technique is not ideal: you have to add an antibiotic cassette
in order to keep selective pressure on the bacteria, so that they integrate the new gene into all
the chromosome copies. This antibiotic resistance will persist in the strain, meaning that when
further engineering the organism later on, this one resistance can not be used e.g. in vectors for
transient expression - a huge downside. Furthermore, one of the neutral sites has to be used,
resulting in a strain that has less neutral sites available for further introduction of genes.
Although we did not prefer this method, we still tried it, as we were not sure, if our other
approach
would prove to be successful. We also used extensive bioinformatic tools to identify new integration sites in UTEX 2973, which can be used if one were to reintroduce
natural
competence in the above mentioned way.
Additionally, we came up with a plan to revert the point mutation in the pilN gene with a
CRISPR/Cas12a
system.
This approach is promising, as the integration of the new pilN copy only enabled a low
efficiency
of
natural transformation, which might be due to the point mutation negatively affecting expression of
the
pil0 and pilQgenes laying downstream of pilN (Li et al., 2018 ; Barten and
Lill, 1995) . As CRISPR/Cas12a allows accurate targeting of genetic sequences, we designed
a crRNA leading the Cas12a protein to the pilN locus. The repair template was taken from
the S.
elongatus PCC 7042 genome, where
the gene is still intact, allowing the cell to repair the cut introduced by Cas12a accordingly,
reversing the point mutation, which leads to an intact copy of pilN again - a more
elegant
approach than
simply inserting a second copy of the gene.
As our own CRISPR system was still in building at that point, we had to rely on pSL2680, a
replicating
base vector for constructing CRISPR/Cas12a editing plasmids by
Ungerer and Pakrasi, 2016 .
We followed their protocol (available here on
Addgene) , annealing oligos to construct the crRNA. Small overhangs were added to
enable the ligation into the AarI-digested vector, where a lacZ
cassette was replaced, which allowed for blue/white screening of recombinant colonies.
This
cloning
step alone took approximately a week. Additionally, the repair template had to be
constructed by PCR
with added overhangs for the following Gibson reaction. As stated, it was taken from the
S.
elongatus PCC 7942 genome. It was designed in such a way that the point mutation
inside the UTEX
2973 genome was part of the PAM sequence for Cas12a, meaning that the repair template
did
not
include the PAM and would not be cut by the enzyme.
CRISPR gene editing)
CRISPR/Cas systems are powerful tools that have gained a lot of popularity in the recent years.
As they can be used for a wide array of applications - like the integration of whole genes, alteration of single
nucleotides, knock-outs of whole genetic regions, as well as the use of the DNA-binding property in a multitude
of applications through so called deadCas systems, where the Cas protein does not exhibit nuclease activity
(Hsuet al., 2014) - we were
eager to implement such a system into our own toolbox.
Diving into the literature we noticed many different systems are available,the most commonly used one being
CRISPR/Cas9, and we began to wonder which of them we should use.
In our description we presented CRISPR/Cas9 and CRISPR/Cas12a,
showing the
differences of these two systems. Looking deeper into CRISPR/Cas12a we noticed a few advantages that finally
led us to choose it as our preferred system.
As the sgRNA used as a guide for Cas9 is usually ~100nt long, chemical synthesis is more complex and
expensive in comparison to the ~43nt needed for the Cas12a guiding crRNA (Swarts and Jinek, 2018) - an
unpleasant fact, especially for iGEM teams that do not have many resources available to them, but the
main reasons we chose Cas12a are others. Multiplexed gene editing is one of the key features of these
CRISPR/Cas systems, but how to actually apply it differs:
For Cas9 each sgRNA is in need of its own promoter, which means that they have to be expressed from
different vectors or a multi cassette vector ( X. Ma et al.,
2015 ; Z.
Zhang et al., 2016 ). In contrary, multiplexed genome editing with Cas12a can be achieved
simply by expressing all of the needed guide RNAs in one transcriptional unit, where they are then
processed into different crRNAs by Cas12a (Kim, et al.,
2016; Nishimasu et al., 2017) . This is a huge advantage of Cas12a. Furthermore, CRISPR/Cas9
was shown to be toxic in cyanobacteria (Wendt et
al., 2016) , which is one of the foremost reasons CRISPR technologies have not been widely
applied in cyanobacteria - the usage of Cas12a though, does not seem to have the same toxicity Ungerer and Pakrasi, 2016 , making it the ideal
candidate for the Green Extension of the Marburg Collection.
The actual implementation of the CRISPR/Cas12a system into our toolbox necessitated a well thought
out plan.
The design of our CRISPR/Cas12a system was mainly affected by the fact that we wanted to have a
convenient and rapid tool for genomic manipulation.
The lvl 0 part (What are parts? Read more about it click here!) of the Cas12a protein was created via PCR amplification from the plasmid
pSL2680, but special overhangs were added in order to clone the PCR product into a lvl 0
acceptor vector. The part was introduced as a coding sequence (CDS) part in the MoClo
standard to be included in the Green Expansion of the Marburg Collection. The lvl 1 part of
the Cas12a protein was equipped with a rather weak promoter so that the toxicity caused by
overproduction of the endonuclease could be kept low. The parts used for lvl 1 assembly
were: pMC0_1_03 + pMC0_2_03 + pMC0_3_07 + pMC0_4_33 + pMC0_5_07 + pMC0_6_17. For the
construction of the crRNA part the design of the plasmid pSL2680 was mainly maintained, but
the lacZ cassette was replaced by a GFP cassette to enable easier screening of crRNA
assembly and to
reduce expenses for X-Gal/IPTG. It was constructed as a part reaching from the RBS site to
the end
of the terminator site. As the whole system is built for modular cloning in PhytoBrick
syntax, it is possible to freely exchange the parts around the Cas12a and crRNA parts - in
this way the amount of crRNA/Cas12a can be controlled by choosing promoters with different
strengths.
Our initial plan was to synthesize the crRNA with the desired overhangs, but as the sequence
contains multiple direct repeats, it was not possible for providers to synthesize this
construct, which is why we split it into four different parts that then had to be assembled.
For this assembly the four parts were first cloned into the pJET1.2/blunt vector by Thermo
Scientific and then digested with BsaI while the acceptor vector was digested with BsmBI. In
this way the final vector still contains BsaI recognition sites, so that it can be used in a
level 1 assembly Golden Gate reaction. The cloning of the level 2 part with this crRNA part
was done by ending with a ligation step to make sure the GFP dropout remains in the vector.
Cyanobacterial shuttle vectors
Following our dream to create the most versatile, MoClo compatible shuttle vector for cyanobacteria we made sure
to pay attention to detail.
When creating new shuttle vectors, one of the most important points to consider is the replication element that
is being used, mainly due to the wanted copy number and a phenomenon called plasmid incompatibility.
Plasmids harboring the same replication or partitioning system can often not be stably maintained in a cell -
they are incompatible (Novick and Hoppenstaedt, 1978) .
With multiple different plasmids bearing the same replication elements, the replication machinery will
randomly choose which plasmids to replicate, leading to one of the different plasmids being copied more
frequently than the other (Thomas, 2014) . As we used the minimal replication element from
the pANS plasmid of S. elongatus in our shuttle-vectors, in
order to have a native origin of replication, we had to consider such plasmid incompatibilities and made sure to
cure our strain of the endogenous pANS - which we could successfully prove.
The next step was the creation of our own, modular shuttle vector.
For this we had to pay attention, as we had to fit it to the PhytoBrick standard in order to use it in our Green
Extension of the Marburg Collection. This means that we had to remove some restriction enzyme cutting sites at
multiple points in the sequence: In repB and repA - both a CDS of the minimal replication element needed for the
vector - lay one BsaI recognition site each, which were removed by introducing a silent point mutation. This
point mutation, in both cases, introduced a synonym codon for glutamic acid, so they should not cause any issues
later on.
A BsmBI site was found within the non-coding sequence of the minimal replication element, meaning that this had
to be changed with a more careful approach, as any change could have heavy influence on secondary structure and
potentially impair the function. Due to this reason we made sure to try all possible variants of mutations to
remove the recognition site of the restriction enzyme
In order to assemble our desired part we synthesized different parts of it with the mutations we introduced. Due
to the length and complexity of the sequence we had to divide the synthesis of the minimal replication element
into three parts that later had to be fused together.
Additionally, we wanted to implement a reporter for easy selection. We chose rfp, which was amplified out of the
Lvl0_8_Amp/ColE1 part from last years Marburg Collection in addition with the ColE1 ori that can be found on it.
This means that our vector does not just contain the cyanobacterial ori of our strain, but also a high copy
origin for replication in E. coli (Gerhart et al., 2002) .
As an antibiotic cassette we chose spectinomycin, which we also amplified by PCR, this time from pAM4787
(Chen et al., 2016) .
Finally, those five fragments - the three parts of the minimal replication element, the ColE1 ori & rfp cassette and the spectinomycin resistance
cassette (aadA) - were fused together in a Gibson reaction, resulting in BBa_K3228069 (sometimes also called lvl
1 ori), the first cyanobacterial shuttle vector for cloning lvl 1 constructs in a modular way. This part has two
BsaI sites that flank the rfp cassette, so that this genetic element will be exchanged with the other parts in a
lvl 1 Golden Gate reaction.
The Marburg Collection: a recap
The Marburg Collection is a toolbox from last year’s iGEM Marburg team for the rational design of metabolic pathways and genetic circuits or any other DNA construct. Thanks to its flexible design based on the ‘Dueber toolbox’ design from Lee et. al (2015) it can be used in a multitude of chassis: since it complies with the PhytoBrick standard, it can even be extended to eukaryotic chassis such as plants. The design of the toolbox is rather simple and user friendly: LVL 0 parts are the basic foundation of every assembly. They contain a single genetic element such as a promoter or terminator. Up to 8 LVL 0 parts are used to build a LVL1 plasmid containing a single transcription unit. Up to 5 of these transcription units can be assembled together in a LVL 2 plasmid (Lee et. al (2015)).
Design of placeholders
Here we present a new feature of the Marburg Collection 2.0: Placeholders. These parts make it possible to construct
plasmids with a placeholder, which can be later on exchanged with any part of the same type.
A key feature in our
expansion is the addition of placeholders that allow high throughput assembly of plasmids that only differ in one part.
A promoter placeholder for example is built into a LVL 1 construct at the promoter position. Instead of a promoter however
it contains a GFP cassette and reversed BsaI cutting sites. This allows BsaI cleavage and removal of the GFP cassette even
after assembly, due to the fact that the BsaI recognition site is not removed from the placeholder.
After that any promoter of choice can be inserted at that position. After ligation, no BsaI cutting sites remain on the vector, so in the end mainly the newly assembled remains. These steps also happen in a one pot one step reaction just like any other Golden Gate assembly.
White green selection under UV light can be used to determine the colonies with the right plasmid: green ones still contain the plasmid with a placeholder, white ones contain the desired vector.
Available Placeholders
Placeholders exist for every position from 1-6, but technically placeholders can also span multiple positions to insert multiple parts at once. For example a placeholder for the position promoter and RBS could be replaced with any combination of promoter and RBS that is deemed right for a specific application. This however would then be a three part assembly. The application of such parts is so narrow that we decided to build the most useful ones. Thanks to its clever design the construction of more placeholder is so simple that it can be done by the user himself with a single site directed mutagenesis of a flank.
Design of the first panS based MoClo compatible shuttle vector
The heart piece of green expansion is BBa_3228069, a LVL 0 part containing origins of replication for E. coli and S. elongatus as well as a spectinomycin cassette. It resembles a type 7+8 (antibiotic cassette + ori) composite part and can be seen as the cyanobacteria specific LVL1 entry vector. Another version of this entry vector contains a kanamycin cassette and BsmbI cutting sites and can be used as the LVL2 entry vector. Just like in our LVL 0 entry vectors for basic parts, we prompted for a fluorescence based reporter in the dropout, rather than lacZ for blue/white screening. Therefore both vectors contain an RFP dropout to signal an insertion. Using this vector in our updated Golden Gate assembly protocols, we achieve a rate of about 9:1 white to red colonies, showing that the assembly is rather efficient.
Designing the characterization of BioBricks
Here we present the design of the plasmids and the workflow used to characterize BioBricks.
In order to
characterize BioBricks they need to be inserted into a measurement vector that is stably maintained in cyanobacteria.
The design of the plasmids to characterize our parts was an amazing experience as it was one of the first times that we
acted not only as creators but also as users of our toolbox. Therefore design of the workflow and design of new parts was
tied together very closely.
The criteria that the measurement vectors need to meet are some of the most basic principles
of Synthetic Biology:
In order to be comparable, all of the constructs must be almost identical and only differ in the
part to be tested. Instead of building each construct independently we utilized our placeholders
(See Results: placeholder)
to build all measurement plasmids for the same type of part from the same blueprint.
We present a set of measurement
entry vectors for the characterization of BioBricks in cyanobacteria (Part range BBa_K3228073 to BBa_K3228075 as well as
BBa_K3228090). They contain our MoClo compatible shuttle vector for cyanobacteria BBa_K3228069 and are therefore the only
MoClo based vector for the characterization of BioBricks in cyanobacteria. These pre assembled LVL 1 plasmids contain a
placeholder for their respective BioBrick type that acts as a Dropout to quickly and effortlessly insert any part of the
same type for an easy characterization. In our results
we show how these measurement entry vectors can save a lot of effort and money when characterizing a greater library of parts.
Additionally, the usage of the same entry vector for each measurement will aid in greater comparability and reproducibility.
For greater comparability across other data sets we decided to use similar BioBricks as in measuring the toolbox for
Vibrio natriegens in the last year. The design from there on was pretty straight forward for promoter and RBS.
For terminators however the design is a bit more intricate: a terminator is not measured in its activity but
rather in its isolative power. Hence, a strong terminator should result in a weak signal. On top of that, measuring
the activity both upstream and downstream of the terminator with two independent reporters would give insight on the
exact transcriptional activity around the area of the terminator
(Chen et al., 2013),
resulting in the most accurate results in respect to the molecular dynamics of a terminator
(See: modeling).
A LVL 2 plasmid was logically the easiest way to construct such a part. We designed a normal LVL 1 plasmid containing
an mTurqouise reporter and a secondary LVL 1 plasmid containing an YFP reporter but missing a promoter.
The fraction of the signal strength of YFP and mTurquoise describe the isolative capacity of the terminator best
(Chen et al., 2013).
This way of calculating isolative
strength is also used in RNA-seq to determine the strength of terminators.
Modular Engineering of Genome Areas (M.E.G.A.)
Here we represent an expansion to the Marburg Collection 2.0: M.E.G.A. – a set of parts for the genomic integration of genes in Synechococcus elongatus UTEX2973 and other cyanobacteria that can be easily extended to other chassis. This set includes parts with homologous flanks for homologous recombination as well as a necessary set of new terminators and antibiotic resistances.
Finding new artificial Neutral integration Site options (a.N.S.o.)
Artificial neutral integration Site options (aNSo) for our purpose in Synechococcus elongatus needed to fulfil
three criteria, to be genuinely considered as potential candidates.
A highly precise algorithm was implemented in a
Python script to find these potential candidates
(link to modeling)
by describing the following criteria. First, no gene
and transcription start site (TSS), i.e. no CDS, was allowed to be disturbed, assuring that no lethal modification was
created by integration. Thereby, we searched for intergenic regions where no TSS had been identified, with a length of at
least 500 bp. These sequences had to be extended in both 3’ and 5’ direction up to a length of at least 2500 bp providing
flanks to ensure the integration by homologous recombination, which should be performed in the lab subsequently. In the
middle of these sequences any gene of interest can be inserted, which gets integrated into the genome by the mentioned
homologous recombination, due to homologous flanks. Second, integration site sequences were not allowed to contain
restriction sites that interfere with the iGEM standards to simplify the cloning process and make them more cross
compatible. All sequences that contained such restriction site were discarded. Executing this newly developed and
unique algorithm resulted in two unique aNSo's within the genome of S. elongatus.
Design neutral integration sites
For a successful homologous integration the sequence to be integrated needs to be flanked by two integration
sites homologous to the neutral site on the target genome. Additionally, the integrated sequence needs to contain an
appropriate selection marker to be able to select for integration events.
It is included in the syntax of the Marburg Collection, that the positions 1 and 6 can not only be used for connectors but
for integration sites as well. Since integration sites contain a BsmBI restriction site just like a connector part,
their construction is a bit more intricate than a normal part:
- Step1: Find your integration site. For more on this see Modeling: integration sites
- Step 2: Determine your two homology sequence. Optimally the two sequences should span around
800-1200 and not begin or end in an ORF. Leave 40 bp of space in a region without an ORF
between the two sequences, this increases the likelihood for successful recombination events.
Note that these bases will be knocked out in the recombination event. - Step 3: Amplify both integration sites via a genomic PCR using the overhang primers for 5’Connectors (upstream homology sequence) and 3’Connectors (downstream homology sequence), respectively. Check if your PCR worked with a test agarose gel.
- Step 4: Purify your PCR sample using any commercial kit to remove genomic DNA.
- Step 5: digest your PCR sample with BsaI (Note that this is uncommon for LVL 0 Cloning but necessary because of the internal BsmBI restriction site)
- Step 6: Digest your LVL 0 Entry vector with BsmBI and purify it over an agarose gel to remove the GfP Dropout.
- Step 7: Ligate your digested PCR sample and LVL 0 Entry vector overnight.
- Step 8: Transform your ligation as usual in an E. coli or V. natriegens strain for cloning. Thanks to the predigested LVL 0 entry vector most colonies should appear white. Pick a few colonies and verify the construct inside by sequencing. Usually at least 1 in 2 sequencing results yields the correct construct.
In a LVL 1 construct, the positions 2-5 representing a full transcription unit (promoter, RBS, CDS, terminator) would be integrated into the genome, while positions 7-8 (origin of replication,antibiotic cassette) would be cut off in the recombination event. The issue with this assembly would be that a marker for the selection after integration is completely missing. Hence, we decided to split the position of the terminator in a similar fashion in which C-terminal tags were integrated into the syntax last year:
All terminators of the Marburg Collection were rebuild as "5a" parts similar to C-terminal tags. This allowed to
insert an antibiotic cassette at the position "5b". For this position 4 different antibiotic cassettes were designed.
Our integration sites were also designed as connectors, so it is possible to build a gene cascade with up to 5
genes that can be inserted into a single neutral site. All integration sites function as 5'Con1 and 3'Con5 connectors,
meaning they are always at the beginning of the first and the end of the last gene in a LVL2 construct.
It is important to note for the user that when designing the vector for integration, the origin should not be compatible
with the organism. This way, it enters the organism and then integrates into the genome or disappears as it cannot be
replicated in its new host. Otherwise the vector will be maintained in the transformed organism and it will be rather
complicated to remove it. If there is no compatible origin available. We designed our toolbox so that it can always be
digested with NotI to linearize the integration cassette and extracted it over a gel. In a lot of cases transformations
and homologous recombinations with linear DNA are a lot more efficient. (See results of strain engineering)
Our system offers the integration of up to 5 genes with 4 different selection markers at 5 different integration sites.
Therefore, the integration of up to 20 genes into the UTEX wild type genome is possible.
Fluorescence reporters for characterization of parts
When working in Synthetic Biology, reporter genes such as fluorescence proteins are indispensable elements to characterize BioBricks. For a good characterization a suitable reporter is required. But reporters can be more than just merely a detection tool for transcriptional activity but they can also give a deeper insight into cellular conditions beyond the genetic context. We provide a diverse set of reporters not only for the purpose of describing genetic tools but also for the sensing of a variety of parameters which are crucial for cyanobacteria.
eYFP
| Aequorea victoria | |
| Excitation Maximum (nm) | 515 |
| Emission Maximum (nm) | 527 |
| Extinction Coefficient (M-1 cm-1) | 67,000 |
| Quantum Yield | 0.67 |
| Brightness | 44.89 |
| pKa | 6.9 |
| Maturation (min) | 9.0 |
| Life- span (ns) | 3.1 |
Source: FP Base (EYFP)
eYFP is the mutant of green fluorescent protein naturally occuring in Aequorea victoria. It is a preferred reporter for cyanobacteria as it bypasses the wavelength at which absorption photoactive pigments occurs, resulting in stronger signal overall (Kukolka & M. Niemeyer, 2004).
Fig. 8 - graph showing the absorption spectra of UTEX 2973 in comparison to the emission maximum of YFP.
Additionally, autofluorescence of cyanobacterial cells is rather low at that point, resulting in a stronger signal compared to the background, increasing the resolution of characterizations.
sYFP2 (S.e.)
| Aequorea victoria | |
| Excitation Maximum (nm) | 515 |
| Emission Maximum (nm) | 527 |
| Extinction Coefficient (M-1 cm-1) | 101,000 |
| Quantum Yield | 0.68 |
| Brightness | 68.68 |
| pKa | 6.0 |
| Maturation (min) | 4.1 |
| Life- span (ns) | 2.9 |
Source: FP Base (sYFP2)
sYFP is a superfolded version of YFP. Thanks to faster maturation it leads not only to a twofold signal strength compared to eYFP: the fast maturation also ensures that every transcribed mRNA leads to the same amount of correctly folded fluorescent protein. This makes measurements more robust towards varying cellular contexts.
mTurquoise2 (S.e.)
| Aequorea victoria | |
| Excitation Maximum (nm) | 434 |
| Emission Maximum (nm) | 474 |
| Extinction Coefficient (M-1 cm-1) | 30,000 |
| Quantum Yield | 0.84 |
| Brightness | 25.2 |
| pKa | 4.5 |
| Maturation (min) | 112.2 |
| Life- span (ns) | 3.7 |
Source: FP Base (mTurquoise2)
mTurquoise2 is a brighter fluorescent variant of mTurquoise with faster maturation and a high photostability, making it one of the better for microscopy applications. Thanks to a shifted emission maximum it is possible to detect both, YFP and mTurquoise in single cells with virtually no bleed-through of signal, making it suitable for dual fluorescent protein applications like terminator characterization ( Link to johannas characterization text).
NanoLuc
NanoLuc is a small luminescent reporter with just a molecular weight of 19,5 kDA. This reporter stands out with a signal strength that is orders of magnitude higher than compared traditional luminescent reporters. It is a very small protein and unlike the lux operon it is only a single gene, reducing the metabolic burden onto the host to a bare minimum. Additionally it is not using ATP as a substrate which is a valuable energy resource in cells. This way it does not affect the cellular context and acts as a truly orthogonal reporter.
TeLuc
TeLuc is a triple mutant of NanoLuc. Thanks to a modified substrate binding pocket it is able to use DTZ as a substrate, resulting in a (42 nm) red-shift (from 460 nm to 502 nm peak) of emission. This bypasses the absorption of Chlorophyll A, making it the more suitable reporter for phototrophic organism.
Antares2
Antares2 is a coupled bioluminescence protein consisting of TeLuc and two flanking CyOFP fluorescence reporters. It
abuses the Bioluminescence Resonance Energy Transfer (BRET) to excite CyOFP with the luminescence of TeLuc. This results
in a further red-shift, making it suitable for applications like deep tissue analysis. Additionally, it can be used in
conjunction with NanoLuc thanks to the utilization of two distinct substrates as well as varying emission peaks. Therefore
it is the world’s only dual luminescent detector pair.
Luminescence is a great tool for accurate measurements, but in
the world of biosensors for the detection of cellular conditions only fluorescent reporters are established yet. We present
reporters for the two most important chemical parameters in cyanobacteria: pH and redox status. We saw that the pH of the
media has a significant impact on the growth of the culture (Link to results growth rate), which is previously described
(Kallas, Castenholz et al.). Cyanobacteria are not
equipped to regulate their internal pH very well, yet they still depend on a stable proton gradient to keep up their
photosynthetic machinery (Billini et al.). We present phlurion2, a
reporter that is modulated in its excitation peak by varying ph values.
pHlurion2 (S.e.)
Info Box:
| Aequorea victoria | acidic (pH 5,5) | alkaline (pH 7,5) |
| Excitation Maximum (nm) | 395 | 475 |
| Emission Maximum (nm) | 509 | 509 |
Source: FP Base (pHlurion2)
pHlurion2 is a mutant of GFP2. Its excitation maximum depends on the surrounding pH value. Therefore it can be used
to detect changes in the cellular pH. As described above a biosensor for this parameter could be of great use, especially
in cyanobacteria. (Mahon, 2011)
Another important cellular factor is the internal redox status. During photosynthesis reactive oxygen species (ROS)
are constantly produced as a byproduct. A critical mass of reactive oxygen species leads to serious cell damage and
cell toxicity through chemical alterations of proteins, DNA and lipids. Especially under high light conditions the redox
status becomes a crucial parameter as it can threaten the cellular fitness.
For example, the overexpression of orthogonal thioredoxin peroxidase leads to the degradation of ROS resulting in enhanced
growth of PCC7942, (Kim et al.)
We present rxYFP, a redox-sensitive reporter for cyanobacteria.
rxYFP (S.e.)
| Aequorea victoria | |
| Excitation Maximum (nm) | 515 |
| Emission Maximum (nm) | 527 |
| Extinction Coefficient (M-1 cm-1) | 101,000 |
| Quantum Yield | 0.68 |
| Brightness | 68.68 |
| pKa | 6.0 |
| Maturation (min) | 4.1 |
| Life- span (ns) | 2.9 |
Source: FP Base (sYFP)
rxYFP is a redox-sensitive yellow fluorescent protein deriving from Aequorea victoria GFP. This reporter contains a pair of redox-active Cys residues (Cys149 and Cys202), which are connected through a disulphide bond under oxidative conditions, resulting in a 2.2-fold reduction of the emission peak. This allows to determine the redox potential in the environment which then expressed the output of fluorescence.