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**Team Grenoble-Alpes 2018: Delay before fluorescence apparition and leaky expression after transformation in three Escherichia coli strains**

The main goal of this characterisation was to find out which E. Coli strain was the most effective among three different strains (TOP10, DH5α and BL21), to obtain a rapid and high red fluorescence with pSB1C3-BBa_J04450.
We also studied the influence of adding 0.3mM of IPTG on the RFP expression in these three strains to see if the leak was different between host strains.
Indeed, former iGEM teams had described a leaky expression of fluorescence with this biobrick, which means there was no need to induce expression with iPTG to obtain a high rate of fluorescence.

As we raised the question in the context of our project, we thought it might be useful to know which E. Coli host strain is the better to use depending on the conditions you want. For instance, you might want to strictly control RFP expression and so you will need to reduce the leaky expression at most. On the contrary, you may want to have the highest leak as possible to avoid using IPTG, a need our team encountered for the using of our automated system.

EXPERIMENT

We wanted to test three E. Coli strains usually used in laboratories : DH5α, TOP10 and BL21, to see, in the context of our system, which one would be the host with the fastest and highest production of RFP.
We used a bacterial stock of our own, coming from commercial bacteria cultured and made competent using our protocol <a href="http://2018.igem.org/Team:Grenoble-Alpes/protocols">(see competency protocol here)</a> a few weeks before the experiment and conserved at -80°C.
We made an heat-shock transformation <a href="http://2018.igem.org/Team:Grenoble-Alpes/protocols">(see transformation protocol here)</a> of 23ng pSB1C3-BBa_J04450 in 25μL of each bacterial strains. We then cultured transformed bacteria in 250μL LB broth medium for one hour until they expressed chloramphenicol resistance. Then, 750μL of LB broth was added with chloramphenicol and incubated for one hour. After centrifuging the bacteria for 10 minutes at 5000 rpm, we replaced the old medium by resuspending the bacterial pellet. We also split the samples in half, and put each new samples in 30mL LB broth with chloramphenicol, completed or not with 0.3mM of IPTG.
We then measured red fluorescence (620nm) and O.D._600nm every hour for 27 hours.
NB: We had to do O.D._600nm manually as the TriStar microplate reader wasn’t able to do such measurements. Due to the experiment duration and the limited access to the laboratory, we were not able to make O.D._600nm measurements between 9 hours and 18 hours in the experiment. For the night, we thus launched automatic measurements for fluorescence, but we do not have any O.D._600nm linked to these measurements.

RESULTS

The results are represented in the following figures.
The data presented here start 17 hours or 18 hours after transformation because we didn’t observed any fluorescence until this point. This might be due to the huge culture volume in which we put bacteria (30mL). A huge volumed allowed us to make a long experiment with lots of measurements, but it also diluted a lot the bacteria and their fluorescence.

Figure 1

The first figure shows the fluorescence obtained for each sample, without taking into account the number of bacteria in the sample. These results were useful as a part of our project, as we wanted the highest fluorescence rate with the lowest time of apparition after transformation to improve the sensibility and speed of our detection system, regardless of the corresponding amount of bacteria.
The figure shows that fluorescence obtained with TOP10 E. Coli was a lot higher than the ones obtained with either BL21 or DH5α. 620nm measured fluorescence for TOP10 was twice as high as the one obtained with BL21 and more than 7 times as high as the one for DH5α. We also observed fluorescence a lot sooner with the TOP10 bacteria : 18 hours after transformation versus 23-24 hours with the other strains.
As for the DH5α and BL21 comparison, we can see that DH5α had a much lower fluorescence rate, whereas BL21 gave pretty good results when induced with ITPG.

Figure 2

The second figure represents the fluorescence rate rectified with O.D._600nm measurements. This allows to compare in a more quantitative way the fluorescence obtained, as if for each point, we had the same number of bacteria. It must be noticed that the differences in O.D._600nm were not clearly significative between the samples, which means that we can still compare them as they probably were in the same growing phase. On this figure, we can see that there is no significant difference between the experiment with fluorescence only, so we can make the same observations as in figure 1.

Figure 3

The third and last figure represents the same results as in figure 1, but we made close-ups to better study each strain and the differences between induced and non induced promoter.
For the DH5α, we can see that there is a higher fluorescence rate for 0.3mM IPTG than without induction. However, we can still observe fluorescence without induction, which corresponds to the promoter leak : it represents almost half of fluorescence obtained with IPTG.
For the TOP10, we can see that there is almost no difference between the patterns obtained with or without induction. This means that the promoter leak is so important that IPTG induction is not significantly useful at all : the biobrick may be transformed and the RFP expressed in this host without using IPTG.
For BL21, the difference between induced and non-induced expression is clearly apparent : there is almost no fluorescence without IPTG, whereas expression with induction began to increase exponentially from 23 hours after transformation. This strain appears to be the most effective if you need to reduce the promoter leak as much as possible.

Results showed the differences between E. Coli host strains, which allow variable RFP expression rates, different delays before fluorescence apparition, and also particular responses to induction. The results are summarized in the following table :

E. Coli strain	DH5α	TOP10	BL21
Delay before fluorescence observation	±22 hours	±18 hours	±22 hours
Fluorescence rate with IPTG	Low	Medium	High
Promoter leak	Medium	Extremely high	Extremely low

The delay before fluorescence must be analyzed with caution, as it might have been affected by the huge culture volume compared to the start amount of bacteria.
The fluorescence rate and promoter leak must be further studied in these three strains with higher concentrations of IPTG to see if we would obtain different results.

Team Kingsborough NY 2017

Part of our project involved assessing the risk of escape posed by a genetically modified organism (GMO), especially one being employed in a wastewater treatment facility. Towards this end, we grew E. coli harboring this part (BBa_J04450) as an example GMO in different conditions, some of which mimic the salinity of seawater (typically 3-5% NaCl w/v). Surprisingly, we noticed that while the bacteria could grow on the higher salt media, the expression of RFP was decreased. This was unexpected, as the promoter in this part that drives RFP expression is not characterized as being salt responsive. We further confirmed this result by directly streaking E. coli with this part on different media.

Fig 1: E. coli with BBa_J04450 streaked onto LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. Since LB Miller already contains 1% NaCl w/v, when preparing 500mL of LB Agar another 10g of NaCl was added to the mixture before sterilization. The bacteria was streaked using a sterile toothpick and a parent colony grown under normal conditions. The plates shown are representative of multiple experiments, and display bacteria after 1 day of growth at 37C.

Fig 2: Quantified levels of RFP expression for E. coli with BBa_J04450 grown for 1 day on LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. Images of the plates were taken and the Grayscale, Red, Green, and Blue levels in each image were determined using ImageJ. RFP expression per cell is approximated by the amount of Red color over a set of pixels divided by the level of Green color. This difference is normalized to the maximum value obtained in all experiments. Graph shown is an average of at least 3 separate experiments, error bars represent standard deviation. Differences between LB Miller and 3% NaCl media were shown to be statistically significant using Student's T-Test (p < 0.05).

Bacteria harboring this part not only display decreased RFP expression in high salt, but also appear to grow slower. This was true for media containing 3% NaCl, but even more severe for media with 5% NaCl. However, allowing additional time for growth at high salt does not allow the bacteria to recover the levels of RFP expression seen after 1 day of growth in normal media.

Fig 3: E. coli with BBa_J04450 grown for 1 day on LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% to 5% NaCl. Plates were allowed to grow overnight at 37C for either 1 or 4 days, and photographed against a dark background.

In addition to a response to high salt media, we also wished to observe how RFP expression changes in different genetic backgrounds - namely, in E. coli with the ssrA::Kan-R insertion, which lack tmRNA and trans-translation ribosome rescue. We used part J04450 as a control for experiments with parts K1399010 through K1399013 (ssrA tagged RFP).

Fig 4: E. coli, either wild-type (WT) or trans-translation deficient (ssrA::Kan-R) with BBa_J04450 streaked onto LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. The bacteria was streaked using a sterile toothpick and a parent colony grown under normal conditions. The plates shown are representative of multiple experiments, and display bacteria after 1 day of growth at 37C.

Fig 5: Quantified levels of RFP expression for E. coli, either wild-type (WT) or trans-translation deficient (ssrA::Kan-R) with BBa_J04450 streaked onto LB + Chloramphenicol plates, and/or supplemented with 1mM IPTG. Data analysis carried out the using the same method described in Fig 2. Graph shown is an average of at least 3 separate experiments, error bars represent standard deviation. Differences between LB Miller and 3% NaCl media were shown to be statistically significant using Student's T-Test (p < 0.05).

The tighter regulation of gene expression (no leaky expression at 0mM IPTG) and overall lower steady state level of RFP in the ssrA:Kan-R is not a complete surprise - others have described how LacI is a substrate for the tmRNA tagging system, and that induction of LacI responsive promoters is usually lower in a background that does not feature tmRNA-mediated ribosome rescue. However, previous studies have featured only a difference in the dynamics of gene expression, and did not observe a difference in steady state levels, as we do here (Abo T, 2000)

Team TecCEM 2017

The objective of this characterization was to evaluate the moment of maximum expression of the protein and its behavior with the induction with IPTG taking into account the previous characterizations that RFP is optimally expressed with 20 mM IPTG. The complete protocol can be consulted in: http://2017.igem.org/Team:TecCEM/Improve

Figure 1. Basic steps for RFP characterization followed by team TecCEM

We measured biomass and fluorescence for 8 hours and made the corresponding curves.

Figure 2. Graph of the biomass growth of the induced and non induced cultures of DH5α + BBa_J04450

Figure 3. Statistical analysis of the measures of RFP obtained through 8 hours of induction.

We performed also two different 10% SDS PAGE for visualizing the 26 kDa band corresponding to the Red Fluorescent Protein. Each gel was loaded with the non-induced sample and its induced counterpart. However, during the previous treatment, we did not incubate the samples at 100ºC in the water bath, while we did for the samples of the other gel. By not performing this step, the protein was not denaturalized and was seen under the transilluminator.

Figures 4 and 5. Comparison between RFP expression in DH5𝑎 induced and no induced with IPTG.

In these figures, we can also see that by each hour the expression of this protein and the fluorescence intensity increased over time until the eighth hour, where it is maximum. After the eighth hour, both biomass and fluorescence intensity start de decay, so any other team that wants to use this BioBrick to induce the expression of any interest protein in liquid medium will have the highest yield after eight hours.

Team Grenoble-Alpes 2017

The colonies of bacteria transformed with this plasmid are clearly red under natural light after about 18 hours. Smaller colonies are visibly red under UV. The RFP part does not contain a degradation tag and the RBS is strong. This part is commonly used, but can fail if the system contains LacI or CAP protein. (Informations from iGEM website, "Parts" section, see here http://2017.igem.org/Team:Grenoble-Alpes/Parts).

The promoter of mRFP1 gene in each plasmid is supposed to be inducible (with IPTG) but a strong leak of RFP production could be observed. (fig 1)

Figure 1: Observation of the leak of the promoter. A : Bacteria transformed or not with BBa_J04450 sequence, naked eye, white light. B. Bacteria without mRFP1 gene, excited at 546nm. C. Bacteria with mRFP1 gene, excited at 546nm. Red fluorescence is notable.

Photos of the fluorescence are taken thanks to SnapLab, the biodetection kit of iGEM Grenoble 2017 (fig 2). Figure 2: SnapLab, the detection kit made by Grenoble-Alpes iGEM Team

-> Does IPTG induction bring forward and/or increase RFP production ?
A difference of fluorescence was evaluated, either on the intensity either on the time of apparition of the fluorescence. The following experiment has been designed in this aim.

Results showed IPTG had an importance in RFP production. Indeed, we can see that IPTG allows a shorter rise of fluorescence. It could be interesting to repeat this experience with different IPTG concentrations, to see whether the delay of apparition of the red fluorescence would decrease with a higher amount of inducer.

Team Warwick 2016

This year, our team demonstrated that this part can be triple transformed into the same competent cell while retaining the functionality of all the plasmids. This was demonstrated using pSB1C3, pSB3T5, and pSB4A5.

pSB4A5 is a BioBrick standard vector with a pSC101 replication origin, whilst pSB3T5 has a p15A replication origin. As both of these origins rely on iterons as the negative copy number control, the competition between the plasmids may render them incompatible when in the same cell[1], potentially limiting triple transformation efficiency. However through our experiment we show that the replication origins do not interfere with each other.

To illustrate this, we transferred the triple transformed cells onto plates containing chloramphenicol, tetracycline, and ampicillin, as shown in Figure 1 below. From this plate, we inoculated a single colony into water and streaked this water onto one half of three different plates containing one each of chloramphenicol, tetracycline, and ampicillin. On the other half of the plates, we streaked a colony of top10 cells that had been grown on a streptomycin plate. The results can be seen below in figures 2 and 3. Figure 3 shows the four plates under UV light, clearly showing where colonies have grown. As the triple transformed cells have grown on every single plates and no colonies have grown from the untransformed cells, this shows that plasmid functionality is retained.

Figure 1: Visible light image of triple transformation plated on Chlor-Amp-Tet plate

Figure 2: Visible light image of triple transformation plated on Chlor, Amp, and Tet plates alongside untransformed Top10 cells

Figure 3: UV light image of triple transformation plated on Chlor, Amp, and Tet plates alongside untransformed Top10 clearly showing differences in growth

Team Warwick 2015

Our team considered using this part as part of a system of binding different coloured cells together in order to demonstrate specific cell placement. We characterised this part is order to determine the optimal amount of IPTG required for inducing the gene, and the copy number necessary to express the fluorescence brightly. The results for this can be seen below.

We cloned J04450 into three plasmid with varying copy numbers, in order from highest to lowest copy number they are: pSB1K3, pSB3K3, and pSB4K5. These plasmids were then transformed into electrocompetent MG1655 Z1 cells and grown overnight. THe next morning the cells were refreshed, and different concentrations of IPTG (0uM, 250uM, and 500uM) were added to induce them. For each of the three plasmids in each IPTG concentrations, three biological replicates were made, and when OD600 and RFP absorbance were measured, three technical replicates were made, for a total of 81 copies of the gene grown. The RFP absorbance and OD600 of these cells were measured over 20 hours. The OD600 over time was used to determine at what OD the cells were in steady state. This was then compared to the RFP measured at that time and graphed to show RFP expression per cell.

The graph shows that RFP expression was highest in the pSB1K3 and pSB4K5 plasmids, and that there was little difference in expression between the 250uM and 500uM concentration of IPTG. 0uM IPTG universally showed almost no expression. pSB1K3 should have the highest copy number and pSB4K5 should have the lowest copy number, so it's curious that they both expressed RFP very well. This could be due to a mutation in the pSB4K5 causing it to have a much higher copy number than usual. It is documented here (http://www.ncbi.nlm.nih.gov/pubmed/1283002) that a single point mutation can increase the copy number of a plasmid. The pSB4K5 plasmid we tested has been sent for sequencing in order to determine whether this is the case.

The raw data for this characterisation can be found here:
https://static.igem.org/mediawiki/2015/7/70/Warwick_J04450_raw_data.txt
https://static.igem.org/mediawiki/2015/b/bc/Warwick_J04450_in_pSB1K3_analysed_results.txt
https://static.igem.org/mediawiki/2015/8/8f/Warwick_J04450_in_pSB3K3_analysed_results.txt
https://static.igem.org/mediawiki/2015/5/54/Warwick_J04450_in_pSB4K5_analysed_results.txt
https://static.igem.org/mediawiki/2015/6/64/Warwick_J04450_RFP_OD_analysed_results.txt

Team NRP-UEA_Norwich 2014

Our team has converted this part into a series of four "GoldenGate Flipper modules" that can be used to convert four types of standard part defined in the GoldenGate MoClo Assembly Standard into standard BioBricks. This was done by inserting an inverted pair of BsaI recognition sequences either side of the original RFP reporter part. The flipper reaction is a one-pot, one-step, digestion-ligation GoldenGate cloning reaction. When cloning is successful the colonies become white as the RFP sequence is replaced by the new part. After the reaction is complete, no part of the BsaI recognition sequence will remain between the BioBrick suffix and the part.

Four types of Golden Gate Parts can be converted. The four new parts differ by the identity of the 4 base-pair 5' overhangs produced by digestion with BsaI.

Bba_K1467100 Pro + 5U MoClo Flipper (GGAG-AATG)
Bba_K1467200 CDS1 MoClo Flipper (AATG-GCTT)
Bba_K1467300 3U + Ter MoClo Flipper (GCTT-CGCT)
Bba_K1467400 Transcriptional Unit MoClo Flipper (GGAG-CGCT)

The image below shows the sequences inserted (in orange) between the RFP and the BioBrick prefix and suffix that enable the flipper to accept MoClo Pro+5U parts (which begin GGAG and end AATG) in a one-step digestion-ligation Golden Gate cloning reaction.

Below is an example of a Golden Gate one-step, one-pot cloning reaction with the improved BioBrick BBa_K1467100, where the restriction enzyme, ligase and (intact, uncut) donating and recipient plasmids were all incubated together in a single reaction before transformation into competent E.coli cells. Cloning was very successful as the vast majority of the colonies are white as the RFP sequence was replaced by the new part.

Team OUC-China 2014

This year our team use this part as a reporter gene link with BBa_k1439000. In order to mark our function plasmid. we find some problem about this part. The result shows Part BBa_J04450 didn’t work well as the reporter gene of the plasmid. The expression quantity of RPF is low or even next to zero under the condition of no resistance screening.

Figure1.

Figure1. Top10 strain containing BBa_J04450(pSB1C3).Culture medium contains no chloramphenicol to the left, to the right contains chloramphenicol. Under the same condition，37℃ 12h，RFP didn’t express in the culture medium without chloramphenicol.

Team NRP-UEA_Norwich 2013

Our team improved this part by adding an NdeI restriction site in front of the promoter region, upstream of the RFP gene. This means a restriction digest can be performed and the promoter or RFP gene exchanged to a allow further cloning. Please see part BBa_K1041000

Our aim was to evaluate RFP expression quantity of E. coli. In order to obtain this information, we agreed that the measurement of fluorescence intensity in certain OD values is the best approach. However, fluorescence quenching was a setback which we must overcome for accurate and reliable results. Because, as a result of quenching, fluorescence intensity counts do not give the actual amount of fluorescence expected from a certain OD value. Therefore we employed a curve fitting method suggested by Zhang et. al (2010) which is claimed to take the quenching problem into consideration

Where If is the fluorescence intensity; OD is the cell density; y0 is the offset; A1 is the amplitude; and t1 is the decay constant.
We chose BBa_J04450 for this experiment. And our negative control was again BBa_B0034.
There were nine bacterial concentrations prepared for one to five hours of IPTG induction. (All concentrations were prepared as triplicates.) Then a complete graph of all the induction durations was plotted with the help of the function shown above:

(■) 1 h induced; (●) 2 h induced; (▲) 3 h induced; (▼) 4 h induced; (♦) 5 h induced

As seen in the graph, fluorescence behaves exactly as expected and does not increase linearly with the increased bacterial concentration. However, IPTG induction effect is clear on fluorescence intensity. (Error bars were too small to be visible.)

Finally, the variables A1 and t1 of the fittings of each induction duration were used to obtain a mean fluorescence intensity (MFI) value:

By conducting this experiment, we were able to characterize RFP expression pattern of the part BBa_J04450 in the host Top Ten. Theoretical mean fluorescence intensity reflects the fluorescence quantum efficiency of the fluorophore RFP, and was found to be unrelated to the cell concentration. Since it is obvious from the results we have obtained that change in the OD does not correlate linearly with the change in the fluorescence intensity. Therefore this model proposes a solution to the unpredictability of the fluorescence amount coming from a certain bacterial population.

The characterization was performed by METU-TURKEY 2010 IGEM TEAM.

Applications of BBa_J04450

According to our result in the 1D chloroquine gel electrophoresis (at 2.5 μg/mL), the plasmid with the BBa_J04450 (on pSB1C3 backbone) migrated further compared to a plasmid with a known GBS (from pBR322 plasmid - BBa_K676012) on pSB1C£. At the chloroquine concentration which we used, the more negatively supercoiled plasmid will migrate further while the more relaxed molecules will travel slower through the gel.

So this indicates that the device BBa J04450 might have a potential gyrase binding site which facilitates the introduction of negative supercoils into plasmid compared to pBR322 GBS.

This characterisation was carried out by the UCL iGEM team 2011.

Tianjin iGEM 2012

Originally, we used this BioBrick to express RFP in Group 4. We mutated the Shine-Dalgarno sequence of this BioBrick to make an orthogonal counterpart, BBa_K821001. As shown in the image, No. 4 is the product of this BioBrick, and No.1 is the product of its orthogonal counterpart. The results justified both this BioBrick and our BBa_K821001 worked very well, and expressed considerable amount of protein.

Glasgow iGEM 2011

It was found that the Red fluorescence of this protein was not consistently apparent when expressed in biofilm - although some results were observed. Numerous attempts to transform this construct into E. coli Nissle 1917 cells in a biofilm forming assay were unsuccessful, however, the RPF expressed readily into E. coli Nissle 1917 cells when grown on an agar plate.

The antibiotic resistance was still carried across when the culture was inoculated into the biofilm assay indicating that the plasmid was still present. The cultures were shaken at room temperature overnight.

It was thought that the lack of fluorescence was caused by the anoxic conditions generated by the biofilm assay, which may have resulted in poor folding of the chromophore. These results show that RFP is not the most efficient reporter molecule for biofilm, we would recommend something like iLOV, a new biobrick submitted by the Glasgow iGEM team this year [1].

Glasgow iGEM team 2011

Haynes Lab, 2012

I used BBa_J04450 to demonstrate the expression of RFP in E. coli for a biomedical engineering course at Arizona State University.

Cells: NEB10B
Medium: LB Lennox agar, 100 ug/mL ampicillin
The yellow/green area contains bacteria expressing GFP from BBa_I13522

User Reviews

UNIQa8a3ae54db02eea4-partinfo-00000007-QINU

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Antiquity

This review comes from the old result system and indicates that this part worked in some test.

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Marc.mtk

We've used this part as an alternative to the suicide part p1010 (ccdB) for selecting against cells that have been transformed with a [http://ginkgobioworks.com/support/BioBrick_Assembly_Manual.pdf destination plasmid]. It worked perfectly, and if i might say, it looks smashingly in LB medium ;).

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Karmella

We obtained this part from the Spring 2011 distribution plate. It expresses wonderfully in NEB10B cells from New England Biolabs. It does not express well in the fast-growing strain DH5-alpha Turbo, which we've found doesn't express transgenes very well in general.

Team Westminster_UOW 2016

During our iGEM project we aimed to characterise two parts, BBa_J04450 which is a pSB1C3 plasmid present within the iGEM 2016 kit. We did a series of experiments testing the different expression rates it grows at in XL1-Blue and TOP10. We found that in XL1-blue it showed some but very little expression rate without IPTG in experiment 2.4. This may indicate that there is “leaky” expression of the RFP taking place. It was also found to grow better with the addition of 0.1mM IPTG (experiment 2.5) the RFP expression was much higher in XL1-Blue which was expected as XL1-Blue contains a LacI inhibitor encoded in its genomic DNA. However this raises the question as to why it showed a low level protein expression when un-induced by IPGT. It was found to grow extremely well in a TOP10 strain with or without IPTG which is expected as TOP10 does not contain the inhibitor molecule that is present within XL1-Blue. We grew the plasmid pSB3T5 (BBa_I52001) containing an RFP insert with a p15A replication origin and a tetracycline resistance gene, It showed protein expression at a low rate when un-induced and grown in TOP10 strain providing evidence for it being a low-medium copy number plasmid. We also determined that pSB1C3 (BBa_J04450) cannot grow in a co-culture of both XL1-blue and TOP10, the co-culture results showed little/no expression of the RFP therefore is ineffective at expressing in a co-culture.

Team iTesla-SoundBio 2017

We used BBa_J04450, a popular biobrick among other iGEM teams as a vector to house our inserts. Encountering an abnormally high false positive rate with our transformations, we found this aspect of the plasmid worth investigating. Each step in the process (digesting, ligating, and transforming) compounds inefficiency, reducing the probability of a successful transformation. The false positive rate does not pose a problem for highly efficient events; however, for rare events where ligation efficiency is diminished, the chances of selecting a false positive increase dramatically. To characterize the false positive rate, we sequenced 8 colonies and determined the main causes of false positives.

In this context, we define a false positive result as a white colony that did not contain the desired insert based on sequencing data. Expanding on that, a negative result appeared as a red colony on the plate, and a ‘true positive’ was a white colony that, after sequencing, we learned contained the expected insert. Of the eight colonies we sequenced from two experiments, three were in fact true positives and five were false positives. Three of the false positives had a problem with their backbones and still had RFP (either undigested or religated BBa_J04450). Interestingly, two of the sequences only contained a fragment of the RFP gene.

The 3’ terminal deletion appears similar to a PstI cut site (one of our biobricking restriction enzymes), leading us to consider two hypotheses. First, the backbone plasmid had a mutation adding a PstI cut site in the middle of the RFP coding region. Second, the conditions of our digestion reaction may have elicited star activity allowing PstI to cut incorrectly.

Figure 1:Location of truncation in the RFP gene. Green text highlights PstI restriction site while the green triangle denotes where the truncation occurred. Base pair numbers refer to location in BBa_J04450 part sequence.

There are solutions for these specific cases of false positives. One option is to run a more exhaustive purification gel. A longer run time and lower voltage would form tighter bands and would help differentiate between completely and partially digested backbones, decreasing inefficiency at this step in the cloning process. Another solution is to apply a silent mutation at base pair 1654, decreasing the odds of this sequence being recognized as a cut site.

Figure 2: Location of frameshift mutation

Another false positive attributed to the backbone was caused by a frameshift mutation (Figure 2). These are unavoidable as the error occurred during PCR, so the only option would be to sequence minipreps after transformation, a precaution we already take.

We determined that the final source for false positives was insert related. There was a large-scale truncated inversion of the gene present in our backbone, and its placement infers such a large error in the process that we didn’t see value in investigating further.

Over all two rounds of our transformations and eight sequenced white colonies,three were true positives and five were false positives. Of those false positives, we determined that two plasmids suffered from pstI enzyme promiscuity (on the backbone), one plasmid incurred a frameshift mutation (also on the backbone), and one plasmid experienced an unprecedented truncated inversion with its insert. We determined a few ways to optimize efficiency, and decrease chances of backbone errors specifically; to run purification gels longer and at a lower voltage, therefore decreasing inefficiency during the digestion step, and to apply a silent mutation at base pair 1654, therefore eliminating the chances of a natural cut site being recognized there.

UNIQa8a3ae54db02eea4-partinfo-0000000B-QINU

@@ Line 1: / Line 1: @@
 __NOTOC__
 This experience page is provided so that any user may enter their experience using this part.<BR>Please enter
 how you used this part and how it worked out.
-===Applications of BBa_K3128009===
+== '''Team Grenoble-Alpes 2018: Delay before fluorescence apparition and leaky expression after transformation in three <i>Escherichia coli</i> strains''' ==
+<br>
+<p style="text-align:justify">
+The main goal of this characterisation was to find out which <i>E. Coli</i> strain was the most effective among three different strains (TOP10, DH5&alpha; and BL21), to obtain a rapid and high red fluorescence with pSB1C3-BBa_J04450. <br>
+We also studied the influence of adding 0.3mM of IPTG on the RFP expression in these three strains to see if the leak was different between host strains.<br>
+Indeed, former iGEM teams had described a leaky expression of fluorescence with this biobrick, which means there was no need to induce expression with iPTG to obtain a high rate of fluorescence.<br><br>
+As we raised the question in the context of our project, we thought it might be useful to know which <i>E. Coli</i> host strain is the better to use depending on the conditions you want. For instance, you might want to strictly control RFP expression and so you will need to reduce the leaky expression at most. On the contrary, you may want to have the highest leak as possible to avoid using IPTG, a need our team encountered for the using of our automated system.<br></p>
+<br>
+<FONT size="2"><i>EXPERIMENT</i></FONT><br><p style="text-align:justify">
+We wanted to test three <i>E. Coli</i> strains usually used in laboratories : DH5&alpha;, TOP10 and BL21, to see, in the context of our system, which one would be the host with the fastest and highest production of RFP. <br>
+We used a bacterial stock of our own, coming from commercial bacteria cultured and made competent using our protocol <a href="http://2018.igem.org/Team:Grenoble-Alpes/protocols">(see competency protocol here)</a> a few weeks before the experiment and conserved at -80&deg;C. <br>
+We made an heat-shock transformation <a href="http://2018.igem.org/Team:Grenoble-Alpes/protocols">(see transformation protocol here)</a> of 23ng pSB1C3-BBa_J04450 in 25&mu;L of each bacterial strains. We then cultured transformed bacteria in 250&mu;L LB broth medium for one hour until they expressed chloramphenicol resistance. Then, 750&mu;L of LB broth was added  with chloramphenicol and incubated for one hour. After centrifuging the bacteria for 10 minutes at 5000 rpm, we replaced the old medium by resuspending the bacterial pellet. We also split the samples in half, and put each new samples in 30mL LB broth with chloramphenicol, completed or not with 0.3mM of IPTG.<br>
+We then measured red fluorescence (620nm) and O.D.<sub>600nm</sub> every hour for 27 hours.
+<br>
+<i>NB: We had to do O.D.<sub>600nm</sub> manually as the TriStar microplate reader wasn’t able to do such measurements. Due to the experiment duration and the limited access to the laboratory, we were not able to make O.D.<sub>600nm</sub> measurements between 9 hours and 18 hours in the experiment. For the night, we thus launched automatic measurements for fluorescence, but we do not have any O.D.<sub>600nm</sub> linked to these measurements.</i><br></p>
+<br>
+<FONT size="2"><i>RESULTS</i></FONT><br><p style="text-align:justify">
+The results are represented in the following figures. <br>
+The data presented here start 17 hours or 18 hours after transformation because we didn’t observed any fluorescence until this point. This might be due to the huge culture volume in which we put bacteria (30mL). A huge volumed allowed us to make a long experiment with lots of measurements, but it also diluted a lot the bacteria and their fluorescence.<br></p>
+https://static.igem.org/mediawiki/parts/e/ea/BBa_J04450-Grenoble-Alpes-2018-fluorescence1.png
+<br><p align="center"><i>Figure 1</i></p>
+<br><p style="text-align:justify">
+The first figure shows the fluorescence obtained for each sample, without taking into account the number of bacteria in the sample. These results were useful as a part of our project, as we wanted the highest fluorescence rate with the lowest time of apparition after transformation to improve the sensibility and speed of our detection system, regardless of the corresponding amount of bacteria.<br>
+The figure shows that fluorescence obtained with TOP10 <i>E. Coli</i> was a lot higher than the ones obtained with either BL21 or DH5&alpha;. 620nm measured fluorescence for TOP10 was twice as high as the one obtained with BL21 and more than 7 times as high as the one for DH5&alpha;. We also observed fluorescence a lot sooner with the TOP10 bacteria :  18 hours after transformation versus 23-24 hours with the other strains.<br>
+As for the DH5&alpha; and BL21 comparison, we can see that DH5α had a much lower fluorescence rate, whereas BL21 gave pretty good results when induced with ITPG.
+<br></p>
+https://static.igem.org/mediawiki/parts/7/7b/BBa_J04450-Grenoble-Alpes-2018-fluorescence2.png
+<p align="center"><i>Figure 2</i></p><br>
+<p style="text-align:justify">
+The second figure represents the fluorescence rate rectified with O.D.<sub>600nm</sub> measurements. This allows to compare in a more quantitative way the fluorescence obtained, as if for each point, we had the same number of bacteria. It must be noticed that the differences in O.D.<sub>600nm</sub> were not clearly significative between the samples, which means that we can still compare them as they probably were in the same growing phase.
+On this figure, we can see that there is no significant difference between the experiment with fluorescence only, so we can make the same observations as in figure 1.
+<br></p>
+https://static.igem.org/mediawiki/parts/9/9c/BBa_J04450-Grenoble-Alpes-2018-fluorescence3.png
+<p align="center"><i>Figure 3</i></p><br>
+<p style="text-align:justify">
+The third and last figure represents the same results as in figure 1, but we made close-ups to better study each strain and the differences between induced and non induced promoter.<br>
+For the DH5α, we can see that there is a higher fluorescence rate for 0.3mM IPTG than without induction. However, we can still observe fluorescence without induction, which corresponds to the promoter leak : it represents almost  half of fluorescence obtained with IPTG.<br>
+For the TOP10, we can see that there is almost no difference between the patterns obtained with or without induction. This means that the promoter leak is so important that IPTG induction is not significantly useful at all : the biobrick may be transformed and the RFP expressed in this host without using IPTG.<br>
+For BL21, the difference between induced and non-induced expression is clearly apparent : there is almost no fluorescence without IPTG, whereas expression with induction began to increase exponentially from 23 hours after transformation. This strain appears to be the most effective if you need to reduce the promoter leak as much as possible.<br>
+<br>
+Results showed the differences between E. Coli host strains, which allow variable RFP expression rates, different delays before fluorescence apparition, and also particular responses to induction. The results are summarized in the following table :<br></p>
+<table style="border: 1px solid black; border-collapse:collapse;">
+<tr>
+  <th style="border: 1px solid black;"><i>E. Coli</i> strain</th>
+  <td style="border: 1px solid black;">DH5&alpha;</td>
+  <td style="border: 1px solid black;">TOP10</td>
+  <td style="border: 1px solid black;">BL21</td>
+</tr>
+<tr>
+  <th style="border: 1px solid black;">Delay before fluorescence observation</th>
+  <td style="border: 1px solid black;">&plusmn;22 hours</td>
+  <td style="border: 1px solid black;">&plusmn;18 hours</td>
+  <td style="border: 1px solid black;">&plusmn;22 hours</td>
+</tr>
+<tr>
+  <th style="border: 1px solid black;">Fluorescence rate with IPTG</th>
+  <td style="border: 1px solid black;">Low</td>
+  <td style="border: 1px solid black;">Medium</td>
+  <td style="border: 1px solid black;">High</td>
+</tr>
+<tr>
+  <th style="border: 1px solid black;">Promoter leak</th>
+  <td style="border: 1px solid black;">Medium</td>
+  <td style="border: 1px solid black;">Extremely high</td>
+  <td style="border: 1px solid black;">Extremely low</td>
+</tr>
+</table>
+<p style="text-align:justify">
+The delay before fluorescence must be analyzed with caution, as it might have been affected by the huge culture volume compared to the start amount of bacteria. <br>
+The fluorescence rate and promoter leak must be further studied in these three strains with higher concentrations of IPTG to see if we would obtain different results.
+</p>
+== '''Team Kingsborough NY 2017''' ==
+Part of our project involved assessing the risk of escape posed by a genetically modified organism (GMO), especially one being employed in a wastewater treatment facility. Towards this end, we grew <i>E. coli</i> harboring this part (BBa_J04450) as an example GMO in different conditions, some of which mimic the salinity of seawater (typically 3-5% NaCl w/v). Surprisingly, we noticed that while the bacteria could grow on the higher salt media, the expression of RFP was decreased. This was unexpected, as the promoter in this part that drives RFP expression is not characterized as being salt responsive. We further confirmed this result by directly streaking <i>E. coli</i> with this part on different media.
+[[File:T--Kingsborough_NY--J04450_fig1.png|800px]]
+<i>Fig 1: E. coli with BBa_J04450 streaked onto LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. Since LB Miller already contains 1% NaCl w/v, when preparing 500mL of LB Agar another 10g of NaCl was added to the mixture before sterilization. The bacteria was streaked using a sterile toothpick and a parent colony grown under normal conditions. The plates shown are representative of multiple experiments, and display bacteria after 1 day of growth at 37C.</i>
+[[File:T--Kingsborough_NY--J04450_fig2.png|800px]]
+<i>Fig 2: Quantified levels of RFP expression for E. coli with BBa_J04450 grown for 1 day on LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. Images of the plates were taken and the Grayscale, Red, Green, and Blue levels in each image were determined using ImageJ. RFP expression per cell is approximated by the amount of Red color over a set of pixels divided by the level of Green color. This difference is normalized to the maximum value obtained in all experiments. Graph shown is an average of at least 3 separate experiments, error bars represent standard deviation. Differences between LB Miller and 3% NaCl media were shown to be statistically significant using Student's T-Test (p < 0.05).</i>
+Bacteria harboring this part not only display decreased RFP expression in high salt, but also appear to grow slower. This was true for media containing 3% NaCl, but even more severe for media with 5% NaCl. However, allowing additional time for growth at high salt does not allow the bacteria to recover the levels of RFP expression seen after 1 day of growth in normal media.
+[[File:T--Kingsborough_NY--J04450_fig3.png|800px]]
+<i>Fig 3: E. coli with BBa_J04450 grown for 1 day on LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% to 5% NaCl. Plates were allowed to grow overnight at 37C for either 1 or 4 days, and photographed against a dark background.</i>
+In addition to a response to high salt media, we also wished to observe how RFP expression changes in different genetic backgrounds - namely, in <i>E. coli</i> with the ssrA::Kan-R insertion, which lack tmRNA and trans-translation ribosome rescue. We used part J04450 as a control for experiments with parts K1399010 through K1399013 (ssrA tagged RFP).
+[[File:T--Kingsborough_NY--J04450_fig4.png|800px]]
+<i>Fig 4: E. coli, either wild-type (WT) or trans-translation deficient (ssrA::Kan-R) with BBa_J04450 streaked onto LB + Chloramphenicol plates supplemented with 1mM IPTG and/or 3% NaCl. The bacteria was streaked using a sterile toothpick and a parent colony grown under normal conditions. The plates shown are representative of multiple experiments, and display bacteria after 1 day of growth at 37C.</i>
+[[File:T--Kingsborough_NY--RFP_ssrA_fig2.png|800px]]
+<i>Fig 5: Quantified levels of RFP expression for E. coli, either wild-type (WT) or trans-translation deficient (ssrA::Kan-R) with BBa_J04450 streaked onto LB + Chloramphenicol plates, and/or supplemented with 1mM IPTG. Data analysis carried out the using the same method described in Fig 2. Graph shown is an average of at least 3 separate experiments, error bars represent standard deviation. Differences between LB Miller and 3% NaCl media were shown to be statistically significant using Student's T-Test (p < 0.05).</i>
+The tighter regulation of gene expression (no leaky expression at 0mM IPTG) and overall lower steady state level of RFP in the ssrA:Kan-R is not a complete surprise - others have described how LacI is a substrate for the tmRNA tagging system, and that induction of LacI responsive promoters is usually lower in a background that does not feature tmRNA-mediated ribosome rescue. However, previous studies have featured only a difference in the dynamics of gene expression, and did not observe a difference in steady state levels, as we do here ([https://www.ncbi.nlm.nih.gov/pubmed/10899129 Abo T, 2000])
+== '''Team TecCEM 2017''' ==
+The objective of this characterization was to evaluate the moment of maximum expression of the protein and its behavior with the induction with IPTG taking into account the previous characterizations that RFP is optimally expressed with 20 mM IPTG. The complete protocol can be consulted in: http://2017.igem.org/Team:TecCEM/Improve
+https://static.igem.org/mediawiki/2017/f/f2/TEC-CEM_Kinectics.GIF
+Figure 1. Basic steps for RFP characterization followed by team TecCEM
+We measured biomass and fluorescence for 8 hours and made the corresponding curves.
+https://static.igem.org/mediawiki/2017/1/1a/TEC-CEM_IPTG_Induction_Curve.GIF
+Figure 2. Graph of the biomass growth of the induced and non induced cultures of DH5α + BBa_J04450
+https://static.igem.org/mediawiki/2017/3/3e/TEC-CEM_RFP_Measurement.GIF
+Figure 3. Statistical analysis of the measures of RFP obtained through 8 hours of induction.
+We performed also two different 10% SDS PAGE for visualizing the 26 kDa band corresponding to the Red Fluorescent Protein. Each gel was loaded with the non-induced sample and its induced counterpart. However, during the previous treatment, we did not incubate the samples at 100ºC in the water bath, while we did for the samples of the other gel. By not performing this step, the protein was not denaturalized and was seen under the transilluminator.
+https://static.igem.org/mediawiki/2017/4/48/TEC-CEM_Comparacion_A.GIF
+https://static.igem.org/mediawiki/2017/c/c8/TEC-CEM_Comparacion_B.GIF
+Figures 4 and 5. Comparison between RFP expression in DH5𝑎 induced and no induced with IPTG.
+In these figures, we can also see that by each hour the expression of this protein and the fluorescence intensity increased over time until the eighth hour, where it is maximum.
+After the eighth hour, both biomass and fluorescence intensity start de decay, so any other team that wants to use this BioBrick to induce the expression of any interest protein in liquid medium will have the highest yield after eight hours.
+== '''Team Grenoble-Alpes 2017''' ==
+The colonies of bacteria transformed with this plasmid are clearly red under natural light after about 18 hours. Smaller colonies are visibly red under UV. The RFP part does not contain a degradation tag and the RBS is strong. This part is commonly used, but can fail if the system contains LacI or CAP protein. (Informations from  iGEM website, "Parts" section, see here http://2017.igem.org/Team:Grenoble-Alpes/Parts).
+The promoter of mRFP1 gene in each plasmid is supposed to be inducible (with IPTG) but a strong leak of RFP production could be observed. (fig 1)
+https://static.igem.org/mediawiki/2017/8/87/Igemgrenoble_part_fig1bis.png
+<br>
+Figure 1: Observation of the leak of the promoter. A : Bacteria transformed or not with BBa_J04450 sequence, naked eye, white light. B. Bacteria without mRFP1 gene, excited at 546nm. C. Bacteria with mRFP1 gene, excited at 546nm. Red fluorescence is notable.
+Photos of the fluorescence are taken thanks to SnapLab, the biodetection kit of iGEM Grenoble 2017 (fig 2).
+https://static.igem.org/mediawiki/2017/4/48/Igemgrenoble_partfig2.png
+Figure 2: SnapLab, the detection kit made by Grenoble-Alpes iGEM Team
+-> Does IPTG induction bring forward and/or increase RFP production ?
+<br>
+A difference of fluorescence was evaluated, either on the intensity either on the time of apparition of the fluorescence. The following experiment has been designed in this aim.
+https://static.igem.org/mediawiki/2017/7/72/Igemgrenoble_diapo1.png
+https://static.igem.org/mediawiki/2017/b/b8/Igemgrenoble_diapo2.png
+https://static.igem.org/mediawiki/2017/0/01/Igemgrenoble_diapo3.png
+Results showed IPTG had an importance in RFP production. Indeed, we can see that IPTG allows a shorter rise of fluorescence. It could be interesting to repeat this experience with different IPTG concentrations, to see whether the delay of apparition of the red fluorescence would decrease with a higher amount of inducer.
+== '''Team Warwick 2016''' ==
+This year, our team demonstrated that this part can be triple transformed into the same competent cell while retaining the functionality of all the plasmids. This was demonstrated using pSB1C3, pSB3T5, and pSB4A5.
+pSB4A5 is a BioBrick standard vector with a pSC101 replication origin, whilst pSB3T5 has a p15A replication origin. As both of these origins rely on iterons as the negative copy number control, the competition between the plasmids may render them incompatible when in the same cell[1], potentially limiting triple transformation efficiency. However through our experiment we show that the replication origins do not interfere with each other.
+To illustrate this, we transferred the triple transformed cells onto plates containing chloramphenicol, tetracycline, and ampicillin, as shown in Figure 1 below. From this plate, we inoculated a single colony into water and streaked this water onto one half of three different plates containing one each of chloramphenicol, tetracycline, and ampicillin. On the other half of the plates, we streaked a colony of top10 cells that had been grown on a streptomycin plate. The results can be seen below in figures 2 and 3. Figure 3 shows the four plates under UV light, clearly showing where colonies have grown. As the triple transformed cells have grown on every single plates and no colonies have grown from the untransformed cells, this shows that plasmid functionality is retained.
+https://static.igem.org/mediawiki/2016/8/84/T--Warwick--ImprovImage1.jpg
+Figure 1: Visible light image of triple transformation plated on Chlor-Amp-Tet plate
+https://static.igem.org/mediawiki/2016/1/10/T--Warwick--ImprovImage2.jpg
+Figure 2: Visible light image of triple transformation plated on Chlor, Amp, and Tet plates alongside untransformed Top10 cells
+https://static.igem.org/mediawiki/2016/2/28/T--Warwick--ImprovImage3.jpg
+Figure 3: UV light image of triple transformation plated on Chlor, Amp, and Tet plates alongside untransformed Top10 clearly showing differences in growth
+== '''Team Warwick 2015''' ==
+<p>
+Our team considered using this part as part of a system of binding different coloured cells together in order to demonstrate specific cell placement. We characterised this part is order to determine the optimal amount of IPTG required for inducing the gene, and the copy number necessary to express the fluorescence brightly. The results for this can be seen below.
+</p>
+<p>
+We cloned J04450 into three plasmid with varying copy numbers, in order from highest to lowest copy number they are: pSB1K3, pSB3K3, and pSB4K5. These plasmids were then transformed into electrocompetent MG1655 Z1 cells and grown overnight. THe next morning the cells were refreshed, and different concentrations of IPTG (0uM, 250uM, and 500uM) were added to induce them. For each of the three plasmids in each IPTG concentrations, three biological replicates were made, and when OD600 and RFP absorbance were measured, three technical replicates were made, for a total of 81 copies of the gene grown. The RFP absorbance and OD600 of these cells were measured over 20 hours. The OD600 over time was used to determine at what OD the cells were in steady state. This was then compared to the RFP measured at that time and graphed to show RFP expression per cell.
+</p>
+https://static.igem.org/mediawiki/2015/8/80/Warwick_J04450_Characterisation_graph.png
+<p>
+The graph shows that RFP expression was highest in the pSB1K3 and pSB4K5 plasmids, and that there was little difference in expression between the 250uM and 500uM concentration of IPTG. 0uM IPTG universally showed almost no expression. pSB1K3 should have the highest copy number and pSB4K5 should have the lowest copy number, so it's curious that they both expressed RFP very well. This could be due to a mutation in the pSB4K5 causing it to have a much higher copy number than usual. It is documented  here (http://www.ncbi.nlm.nih.gov/pubmed/1283002) that a single point mutation can increase the copy number of a plasmid. The pSB4K5 plasmid we tested has been sent for sequencing in order to determine whether this is the case.
+</p>
+<p>
+The raw data for this characterisation can be found here:
+<br> https://static.igem.org/mediawiki/2015/7/70/Warwick_J04450_raw_data.txt
+<br> https://static.igem.org/mediawiki/2015/b/bc/Warwick_J04450_in_pSB1K3_analysed_results.txt
+<br> https://static.igem.org/mediawiki/2015/8/8f/Warwick_J04450_in_pSB3K3_analysed_results.txt
+<br> https://static.igem.org/mediawiki/2015/5/54/Warwick_J04450_in_pSB4K5_analysed_results.txt
+<br> https://static.igem.org/mediawiki/2015/6/64/Warwick_J04450_RFP_OD_analysed_results.txt
+</p>
+== '''Team NRP-UEA_Norwich 2014''' ==
+Our team has converted this part into a series of  four "GoldenGate Flipper modules" that can be used to convert four types of standard part defined in the GoldenGate MoClo Assembly Standard into standard BioBricks. This was done by inserting an inverted pair of BsaI recognition sequences either side of the original RFP reporter part. The flipper reaction is a one-pot, one-step, digestion-ligation GoldenGate cloning reaction. When cloning is successful the colonies become white as the RFP sequence is replaced by the new part. After the reaction is complete, no part of the BsaI recognition sequence will remain between the BioBrick suffix and the part.<br>
+Four types of Golden Gate Parts can be converted. The four new parts differ by the identity of the 4 base-pair 5' overhangs produced by digestion with BsaI.<br>
+Bba_K1467100 Pro + 5U MoClo Flipper (GGAG-AATG)<br>
+Bba_K1467200 CDS1 MoClo Flipper (AATG-GCTT)<br>
+Bba_K1467300 3U + Ter MoClo Flipper (GCTT-CGCT)<br>
+Bba_K1467400 Transcriptional Unit MoClo Flipper (GGAG-CGCT)<br>
+The image below shows the sequences inserted (in orange) between the RFP and the BioBrick prefix and suffix that enable the flipper to accept MoClo Pro+5U parts (which begin GGAG and end AATG) in a one-step digestion-ligation Golden Gate cloning reaction. <br>
+[[Image:Pro flipper.jpg|600px|]]
+Below is an example of a  Golden Gate one-step, one-pot cloning reaction with the improved BioBrick BBa_K1467100, where the restriction enzyme, ligase and (intact, uncut) donating and recipient plasmids were all incubated together in a single reaction before transformation into competent ''E.coli'' cells. Cloning was very successful as the vast majority of the colonies are  white as the RFP sequence was replaced by the new part.
+[[Image:Pro-Flipper Chracterisation.jpg|600px|]]
+== '''Team OUC-China 2014 ''' ==
+This year our team use this part as a reporter gene link with BBa_k1439000. In order to mark our function plasmid. we find some problem about this part. The result shows Part BBa_J04450 didn’t work well as the reporter gene of the plasmid. The expression quantity of RPF is low or even next to zero under the condition of no resistance screening.
+https://static.igem.org/mediawiki/2014/6/6a/OUC-China_J04450.png
+Figure1.
+Figure1. Top10 strain containing BBa_J04450(pSB1C3).Culture medium contains no chloramphenicol to the left, to the right contains chloramphenicol. Under the same condition，37℃ 12h，RFP didn’t express in the culture medium without chloramphenicol.
+<br>
+== '''Team NRP-UEA_Norwich 2013''' ==
+Our team improved this part by adding an NdeI restriction site in front of the promoter region, upstream of the RFP gene. This means a restriction digest can be performed and the promoter or RFP gene exchanged to a allow further cloning. Please see part <partinfo>BBa_K1041000</partinfo>
+<br>
+<br>
+Our aim was to evaluate RFP expression quantity of E. coli. In order to obtain this information, we agreed that the measurement of fluorescence intensity  in certain OD values is the best approach. However, fluorescence quenching was a setback which we must overcome for accurate and reliable results. Because, as a result of quenching, fluorescence intensity counts do not give the actual amount of fluorescence expected from a certain OD value. Therefore we employed a curve fitting method suggested by Zhang et. al (2010) which is claimed to take the quenching problem into consideration
+<br>
+<html> <div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 162px; height: 34px;" alt="w7" src="https://static.igem.org/mediawiki/2010/2/2b/Denklem_1.jpg"></a></div> </html>
+<br>
+<br>   Where If is the fluorescence intensity; OD is the cell density; y0 is the offset; A1 is the amplitude; and t1 is the decay constant.
+<br>   We chose BBa_J04450 for this experiment. And our negative control was again BBa_B0034.
+<br>   There were nine bacterial concentrations prepared for one to five hours of IPTG induction. (All concentrations were prepared as triplicates.) Then a complete graph of all the induction durations was plotted with the help of the function shown above:
+<br>
+<html><div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 400px; height: 280px;" alt="w7" src="https://static.igem.org/mediawiki/2010/9/9b/C7.jpg"></a></div> </html>
+<br> <div align="center">(■) 1 h induced; (●) 2 h induced; (▲) 3 h induced; (▼) 4 h induced; (♦) 5 h induced </div>
+<br>
+<br>    As seen in the graph, fluorescence behaves exactly as expected and does not increase linearly with the increased bacterial concentration. However, IPTG induction effect is clear on fluorescence intensity. (Error bars were too small to be visible.)
+<br>
+<html> <div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 314px; height: 210px;" alt="w7" src="https://static.igem.org/mediawiki/2010/b/b0/Fluorescence_intensity.jpg"></a></div> </html>
+<br>
+<br> Finally, the variables A1 and t1 of the fittings of each induction duration were used to obtain a mean fluorescence intensity (MFI) value:
+<html> <div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 136px; height: 42px;" alt="w7" src="https://static.igem.org/mediawiki/2010/d/d6/MFI.jpg"></a></div> </html>
+<br>
+<html> <div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 300px; height: 280px;" alt="w7" src="https://static.igem.org/mediawiki/2010/c/c2/C8.jpg"></a></div> </html>
+<br>
+<html> <div align="center" style="margin:15px 0px 0px 0px"><img style="border: 0px solid ; width: 266px; height: 135px;" alt="w7" src="https://static.igem.org/mediawiki/2010/3/32/MFI_table.jpg"></a></div> </html>
+<br>
+<br>By conducting this experiment, we were able to characterize RFP expression pattern of the part BBa_J04450 in the host Top Ten. Theoretical mean fluorescence intensity reflects the fluorescence quantum efficiency of the fluorophore RFP, and was found to be unrelated to the cell concentration. Since it is obvious from the results we have obtained that change in the OD does not correlate linearly with the change in the fluorescence intensity. Therefore this model proposes a solution to the unpredictability of the fluorescence amount coming from a certain bacterial population.
+The characterization was performed by METU-TURKEY 2010 IGEM TEAM.
+===Applications of BBa_J04450===
+[[Image:spy.jpg]]
+According to our result in the 1D chloroquine gel electrophoresis (at 2.5 μg/mL), the plasmid with the BBa_J04450 (on pSB1C3 backbone) migrated further compared to a plasmid with a known GBS (from pBR322 plasmid - BBa_K676012) on pSB1C£. At the chloroquine concentration which we used, the more negatively supercoiled plasmid will migrate further while the more relaxed molecules will travel slower through the gel.
+So this indicates that the device BBa J04450 might have a potential gyrase binding site which facilitates the introduction of negative supercoils into plasmid compared to pBR322 GBS.
+This characterisation was carried out by the UCL iGEM team 2011.
+----
+===Tianjin iGEM 2012===
+[[Image:Tianjin1.PNG]]
+Originally, we used this BioBrick to express RFP in Group 4. We mutated the Shine-Dalgarno sequence of this BioBrick to make an orthogonal counterpart, BBa_K821001. As shown in the image, No. 4 is the product of this BioBrick, and No.1 is the product of its orthogonal counterpart. The results justified both this BioBrick and our BBa_K821001 worked  very well, and expressed considerable amount of protein.
+----
+'''Glasgow iGEM 2011'''
+It was found that the Red fluorescence of this protein was not consistently apparent when expressed in biofilm - although some results were observed. Numerous attempts to transform this construct into ''E. coli'' Nissle 1917 cells in a biofilm forming assay were unsuccessful, however, the RPF expressed readily into ''E. coli'' Nissle 1917 cells when grown on an agar plate.
+The antibiotic resistance was still carried across when the culture was inoculated into the biofilm assay indicating that the plasmid was still present. The cultures were shaken at room temperature overnight.
+It was thought that the lack of fluorescence was caused by the anoxic conditions generated by the biofilm assay, which may have resulted in poor folding of the chromophore. These results show that RFP is not the most efficient reporter molecule for biofilm, we would recommend something like iLOV, a new biobrick submitted by the Glasgow iGEM team this year 	[https://parts.igem.org/wiki/index.php?title=Part:BBa_K660004].
+[[Image:Gla_RFP_Dilutions.jpg]]
+[[Image:Gla_RFP_Biofilm.jpg]]
+[[Image:Gla_RFP_Overnight.jpg]]
+[[Image:Gla_RFP_Streakout.jpg]]
+Glasgow iGEM team 2011
+----
+'''Haynes Lab, 2012'''
+I used BBa_J04450 to demonstrate the expression of RFP in E. coli for a biomedical engineering course at Arizona State University.
+* Cells: NEB10B
+* Medium: LB Lennox agar, 100 ug/mL ampicillin
+* The yellow/green area contains bacteria expressing GFP from BBa_I13522
+[[Image:KAH010812.jpg|200px]]
 ===User Reviews===
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+|-
+|width='10%'|
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+<I>Antiquity</I>
+|width='60%' valign='top'|
+This review comes from the old result system and indicates that this part worked in some test.
+|}
+{|width='80%' style='border:1px solid gray'
+|-
+|width='10%'|
+<partinfo>BBa_J04450 AddReview 5</partinfo>
+<I>[[User:Marc.mtk|Marc.mtk]]</I>
+|width='60%' valign='top'|
+We've used this part as an alternative to the suicide part p1010 (ccdB) for selecting against cells that have been transformed with a [http://ginkgobioworks.com/support/BioBrick_Assembly_Manual.pdf destination plasmid]. It worked perfectly, and if i might say, it looks smashingly in LB medium ;).
+|}
+{|width='80%' style='border:1px solid gray'
+|-
+|width='10%'|
+<partinfo>BBa_J04450 AddReview 5</partinfo>
+<I>[[User:Kahaynes|Karmella]]</I>
+|width='60%' valign='top'|
+We obtained this part from the Spring 2011 distribution plate. It expresses wonderfully in NEB10B cells from New England Biolabs. It does not express well in the fast-growing strain DH5-alpha Turbo, which we've found doesn't express transgenes very well in general.
+|}
+== '''Team Westminster_UOW 2016 ''' ==
+During our iGEM project we aimed to characterise two parts,  BBa_J04450 which is a pSB1C3 plasmid present within the iGEM 2016 kit. We did a series of experiments testing the different expression rates it grows at in XL1-Blue and TOP10. We found that in XL1-blue it showed some but very little expression rate without IPTG in experiment 2.4. This may indicate that there is “leaky” expression of the RFP taking place. It was also found to grow better with the addition of 0.1mM IPTG (experiment 2.5) the RFP expression was much higher in XL1-Blue which was expected as XL1-Blue contains a LacI inhibitor encoded in its genomic DNA. However this raises the question as to why it showed a low level protein expression when un-induced by IPGT.  It was found to grow extremely well in a TOP10 strain with or without IPTG which is expected as TOP10 does not contain the inhibitor molecule that is present within XL1-Blue. We grew the plasmid pSB3T5 (BBa_I52001) containing an RFP insert with a p15A replication origin and a tetracycline resistance gene, It showed protein expression at a low rate when un-induced and grown in TOP10 strain providing evidence for it being a low-medium copy number plasmid. We also determined that pSB1C3 (BBa_J04450) cannot grow in a co-culture of both XL1-blue and TOP10, the co-culture results showed little/no expression of the RFP therefore is ineffective at expressing in a co-culture.
+https://static.igem.org/mediawiki/parts/1/16/T--Westminster_UoW--UOW_iGEM_table1.png
+https://static.igem.org/mediawiki/parts/1/14/T--Westminster_UoW--UOW_iGEM_table2.png
+https://static.igem.org/mediawiki/parts/2/2b/T--Westminster_UoW--UOW_iGEM_image1.png
+<br>
+== '''Team iTesla-SoundBio 2017''' ==
+We used BBa_J04450, a popular biobrick among other iGEM teams as a vector to house our inserts. Encountering an abnormally high false positive rate with our transformations, we found this aspect of the plasmid worth investigating. Each step in the process (digesting, ligating, and transforming) compounds inefficiency, reducing the probability of a successful transformation. The false positive rate does not pose a problem for highly efficient events; however, for rare events where ligation efficiency is diminished, the chances of selecting a false positive increase dramatically. To characterize the false positive rate, we sequenced 8 colonies and determined the main causes of false positives.<br>
+<br>In this context, we define a false positive result as a white colony that did not contain the desired insert based on sequencing data. Expanding on that, a negative result appeared as a red colony on the plate, and a ‘true positive’ was a white colony that, after sequencing, we learned contained the expected insert. Of the eight colonies we sequenced from two experiments, three were in fact true positives and five were false positives. Three of the false positives had a problem with their backbones and still had RFP (either undigested or religated BBa_J04450). Interestingly, two of the sequences only contained a fragment of the RFP gene. <br>
+<br>The 3’ terminal deletion appears similar to a PstI cut site (one of our biobricking restriction enzymes), leading us to consider two hypotheses. First, the backbone plasmid had a mutation adding a PstI cut site in the middle of the RFP coding region. Second, the conditions of our digestion reaction may have elicited star activity allowing PstI to cut incorrectly.<br>
+[[File:C99379C4-F58F-4AE3-83E1-6F3DCF818875.png|404px|thumb|center|Figure 1:Location of truncation in the RFP gene. Green text highlights PstI restriction site while the green triangle denotes where the truncation occurred. Base pair numbers refer to location in BBa_J04450 part sequence.]]
+<br>There are solutions for these specific cases of false positives. One option is to run a more exhaustive purification gel. A longer run time and lower voltage would form tighter bands and would help differentiate between completely and partially digested backbones, decreasing inefficiency at this step in the cloning process. Another solution is to apply a silent mutation at base pair 1654, decreasing the odds of this sequence being recognized as a cut site.<br>
+[[File:98685035-7EC6-4B03-97C1-8978FE8D6CAD.png|400px|thumb|left|Figure 2: Location of frameshift mutation]]
+<br>Another false positive attributed to the backbone was caused by a frameshift mutation <i>(Figure 2)</i>. These are unavoidable as the error occurred during PCR, so the only option would be to sequence minipreps after transformation, a precaution we already take.<br>
+<br>We determined that the final source for false positives was insert related. There was a large-scale truncated inversion of the gene present in our backbone, and its placement infers such a large error in the process that we didn’t see value in investigating further.<br>
+<br>Over all two rounds of our transformations and eight sequenced white colonies,three were true positives and five were false positives. Of those false positives, we determined that two plasmids suffered from pstI enzyme promiscuity (on the backbone), one plasmid incurred a frameshift mutation (also on the backbone), and one plasmid experienced an unprecedented truncated inversion with its insert. We determined a few ways to optimize efficiency, and decrease chances of backbone errors specifically; to run purification gels longer and at a lower voltage, therefore decreasing inefficiency during the digestion step, and to apply a silent mutation at base pair 1654, therefore eliminating the chances of a natural cut site being recognized there.<br>
+<!-- DON'T DELETE --><partinfo>BBa_J04450 EndReviews</partinfo>