Understanding how multiple signals are integrated in living cells to produce a balanced response is a major challenge in biology. Two-component signal transduction pathways, such as bacterial chemotaxis, comprise histidine protein kinases (HPKs) and response regulators (RRs). These are used to sense and respond to changes in the environment. Rhodobacter sphaeroides has a complex chemosensory network with two signaling clusters, each containing a HPK, CheA. Here we demonstrate, using a mathematical model, how the outputs of the two signaling clusters may be integrated. We use our mathematical model supported by experimental data to predict that: (1) the main RR controlling flagellar rotation, CheY6, aided by its specific phosphatase, the bifunctional kinase CheA3, acts as a phosphate sink for the other RRs; and (2) a phosphorelay pathway involving CheB2 connects the cytoplasmic cluster kinase CheA3 with the polar localised kinase CheA2, and allows CheA3-P to phosphorylate non-cognate chemotaxis RRs. These two mechanisms enable the bifunctional kinase/phosphatase activity of CheA3 to integrate and tune the sensory output of each signaling cluster to produce a balanced response. The signal integration mechanisms identified here may be widely used by other bacteria, since like R. sphaeroides, over 50% of chemotactic bacteria have multiple cheA homologues and need to integrate signals from different sources.
Chemotactic bacteria sense nutrient gradients and swim towards better environments for growth. A cluster of receptors in the cell membrane detects nutrient levels and signals via a cytoplasmic signaling pathway to the flagellum. The complexity of this signaling pathway varies across different bacterial species. The relatively simple pathway used by Escherichia coli is well understood; however, many bacteria, for example Rhodobacter sphaeroides, have more sophisticated pathways that, as well as being able to detect nutrients, are also able to assess the metabolic state of the cell. The receptors that detect metabolic state are located within an additional cluster that is physically distinct from the one that senses nutrients. In this work, we use a combination of experimentation and mathematical modeling to gain insight into the complex decision-making mechanisms that enable bacteria to weigh-up different stimuli and decide upon an appropriate response. We find novel communication mechanisms between the two signaling clusters that allow the outputs of the signaling pathways to be balanced and tuned according to the prevailing environmental conditions. The signaling principles identified here are likely to be used in other complex sensory networks.
Citation: Tindall MJ, Porter SL, Maini PK, Armitage JP (2010) Modeling Chemotaxis Reveals the Role of Reversed Phosphotransfer and a Bi-Functional Kinase-Phosphatase. PLoS Comput Biol 6(8): e1000896. doi:10.1371/journal.pcbi.1000896
Editor: Christopher V. Rao, University of Illinois at Urbana-Champaign, United States of America
Received: March 14, 2010; Accepted: July 20, 2010; Published: August 19, 2010
Copyright: © 2010 Tindall et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: MJT and SLP were supported by research grant BB/C513350/1 from the Biological and Biotechnology Sciences Research Council (BBSRC). SLP was also supported by the Oxford Centre for Integrative Systems Biology (OCISB). PKM was partially supported by a Royal Society-Wolfson Research Merit award. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Two-component signaling pathways are the major mechanism by which bacterial cells sense and respond to changes in their environment. They regulate processes as diverse as virulence, gene expression, development and motility . Bacteria can have over 100 different two-component pathways per cell, one form of which controls swimming behavior. This chemosensory pathway has been extensively studied as an example of a two-component signaling pathway as it provides a model of signaling, signal termination and receptor adaptation. Mathematical modeling has proved particularly useful in helping to understand the complexity of Escherichia coli chemotaxis –.
Most chemotactic bacteria sense changes in their extracellular environment using transmembrane chemoreceptors . These chemoreceptors signal via an intracellular signaling cascade to the flagellar motor. In the case of E. coli, the signaling cascade is well understood , . The chemoreceptors form a quaternary complex at the cell poles with the scaffold protein CheW and the histidine protein kinase, CheA –. The chemoreceptors detect changes in the periplasmic chemoeffector concentration and control the rate at which CheA autophosphorylates on a conserved histidine residue. In response to decreased attractant concentration, the chemoreceptors signal to increase the rate of CheA autophosphorylation –. Following autophosphorylation, the phosphoryl group is transferred from the histidine residue of CheA to an aspartate residue in one of the two response regulators (RRs), CheY or CheB –. CheY-P is released from the chemotaxis cluster and diffuses through the cell to the flagellar motor. CheY-P binds the FliM component of the flagellar motors, causing the direction of flagellar rotation to switch from counter-clockwise to clockwise resulting in tumbling of the bacterium , . CheA-P also phosphorylates the methylesterase CheB, which facilitates adaptation of the chemoreceptor cluster , . CheY-P and CheB-P both naturally autodephosphorylate , although the rate of CheY-P dephosphorylation is enhanced by CheZ to allow signal termination within the time required for effective gradient sensing , .
In contrast to E. coli, Rhodobacter sphaeroides has a more complex signaling pathway with multiple copies of the signaling proteins encoded by three major chemosensory operons . Many other bacterial species appear to have multiple chemosensory operons as analysis of sequenced genomes suggests that ∼50% of species with any che genes have at least two cheAs –. This raises the question of how behavior is controlled by two or more homologous pathways and how sensory data from each of the pathways are integrated to produce a balanced response. Under laboratory conditions, R. sphaeroides swims using a single sub-polar unidirectional flagellum (Fla1), which is controlled by the protein products of cheOp2 and cheOp3 –. The intracellular signaling cascade controlling the Fla1 flagellum comprises three CheA kinase proteins (denoted CheA2, CheA3, CheA4), three CheY proteins (CheY3, CheY4 and CheY6) and two CheBs (CheB1, CheB2) , , –. CheA3 and CheA4 are unusual CheAs in that they lack some of the domains found in E. coli CheA and neither protein is capable of autophosphorylation . However, together CheA3 and CheA4 have all of the activities of a functional CheA with CheA4 forming a homodimer that binds ATP and phosphorylates the Hpt domain of CheA3.
The signal transduction proteins are organized and localised into two distinct sensory clusters and the signaling output of both clusters is required for chemotaxis , . CheA2 is located in a chemotaxis cluster at the cell poles, which comprises transmembrane chemoreceptors and the signal transduction proteins encoded by cheOp2 . This cluster detects changes in the periplasmic concentration of chemoeffectors. Previous data show that CheA2-P rapidly phosphorylates CheY3, CheY4, CheY6, CheB1 and CheB2 (Figure 1), although the kinetics of phosphotransfer differ in each case . CheA3 and CheA4 localize to a second chemotaxis cluster found in the cytoplasm . This cluster contains the signal transduction proteins encoded by cheOp3 along with the soluble chemoreceptors and is believed to sense the metabolic state of the cell , . CheA3-P rapidly phosphorylates only the RRs, CheY6 and CheB2 , . In addition, CheA3 has an aspartyl-phosphate phosphatase activity that is specific for CheY6-P; this activity is required for the rapid signal termination that is necessary for chemotactic responses . CheA3 in conjunction with CheA4 can therefore be considered to be a bifunctional kinase/phosphatase.
The polar chemotaxis cluster contains CheA2 and responds to the external environment. CheA2 autophosphorylates and can then serve as a phosphodonor for all of the RRs. The cytoplasmic chemotaxis cluster contains CheA3 and CheA4, and is thought to respond to the metabolic state of the cell. CheA3 is phosphorylated by CheA4. Unlike CheA2-P, CheA3-P is not able to phosphorylate all of the RRs – it can only phosphorylate CheY6 and CheB2. All of the RR-Ps spontaneously autodephosphorylate; however, the dephosphorylation of CheY6-P is accelerated by the phosphatase activity of CheA3.
In vitro studies have shown that all of the R. sphaeroides CheYs can bind the flagellar switch protein, FliM, and that this binding is strongest when the CheYs are phosphorylated , but less is known about the effect of CheY/CheY-P binding to FliM on flagellar rotation. CheY6 is essential for chemotaxis and CheY6-P alone is capable of causing the chemotactic stop that is necessary for changing swimming direction . However, CheY6 alone cannot support chemotaxis; either CheY3 or CheY4 are also required. Furthermore, phosphorylation site mutants of CheY3, CheY4 and CheY6 do not support chemotaxis , suggesting that phosphorylation of all of these CheYs is necessary for chemotaxis.
Thus there are two complete chemosensory pathways in R. sphaeroides, localized to different regions of the cell and with different patterns and kinetics of phosphotransfer to the RRs. However, the outputs of these two signaling pathways must be integrated to control the behavior of a single flagellar motor. In vitro biochemistry identified which RRs are phosphorylated by each CheA and the kinetics of the interactions, however, assessing the relative contribution made to RR-P levels by each of these CheAs in vivo is more complex, since all of the RR-Ps will be competing with one another for phosphorylation by the CheAs. We used mathematical modeling to predict the possible signaling pathways within this complex system and tested these predictions experimentally.
The aim of this study was therefore to combine our knowledge of the kinetic preferences of the signaling reactions gained from in vitro biochemistry with the in vivo data on protein copy number within a mathematical model that can predict the changes in RR-P levels resulting from changes in CheA activity at either cluster. This model was then used to analyze the contribution made by each cluster in controlling RR-P levels and the dynamics of the signaling reactions. Using the model, we identified unexpected key roles for reversed phosphotransfer between RR-P and CheA in the network, which would enable communication between the two sensory clusters and thus regulate the output signals. In addition, we demonstrated that the principal RR, CheY6, with the aid of its specific phosphatase, the bifunctional CheA3/CheA4 kinase, could act as a phosphate sink for the other RR-Ps. Regulation of the output of sensory networks by the activity of key kinase/phosphatase proteins is likely to be a common mechanism, but this is one of the first to be identified that balances the outputs of two interconnected pathways.
Construction of the mathematical model
Within an R. sphaeroides cell, CheA2 has been shown to localize to the polar chemotaxis cluster, while CheA3 and CheA4 localize to the cytoplasmic cluster . All the R. sphaeroides CheYs are free to diffuse throughout the cytoplasm of the cell enabling communication between the receptor clusters and flagellar motor. Unlike E. coli, the CheBs are also diffuse in the cytoplasm , . As illustrated in Figure 1, CheA2-P can phosphorylate all of the RRs, whilst CheA3-P is only able to phosphorylate CheY6 and CheB2. What is the reason for this discrimination and how does it contribute towards the chemotactic response of the cell? To understand the role of each signaling cluster we constructed an ordinary differential equation (ODE) model of an R. sphaeroides cell as detailed in Text S1. The model integrates in vivo protein expression levels with in vitro data on the kinetic preference of the CheAs for each of the RRs to predict RR-P levels throughout a simulated chemotactic response. The model includes the phosphorylation reactions shown in Table 1 and was parameterized with published reaction rate constants and protein expression levels (Table 2).
The parameters for the phosphotransfer reactions were obtained by parameter fitting the previously published R. sphaeroides chemotaxis phosphotransfer assay data , , , where CheA-32P served as a phosphodonor to the RRs (Table 3). In the few cases where the assays were not very sensitive to the rate of reversed phosphotransfer from RR-P to CheA, reliable estimates of these rates were obtained using alternative phosphotransfer assays, in which RR-P was mixed with unphosphorylated CheA2 or CheA3 (examples shown in Figure 2). In these reactions, RR-P was generated using purified phosphorylated CheA P1 domains (either CheA2P1-P or CheA3P1-P) as the phosphodonor; control reactions lacking RR showed no phosphotransfer from CheA2P1-P or CheA3P1-P to either CheA2 or CheA3. These experiments showed that while CheA2 is phosphorylated by CheB2-P (Figure 2C) it is not phosphorylated by CheY6-P (Figure 2B). The parameter values obtained from these phosphotransfer reactions were then used in constructing the model.
30 µM CheA3P1-32P was incubated with 5 µM CheA2 for 1 hour prior to the addition of (A) reaction buffer, (B) 10 µM CheY6 and (C) 10 µM CheB2. 10 µl reaction samples were then taken at the time points indicated and quenched in 20 µl of 1.5 X SDS/EDTA loading dye. The quenched samples were analyzed by SDS-PAGE and detected by phosphorimaging.
Response regulator dephosphorylation rates show CheY6 acts as a phosphate sink
R. sphaeroides responds to brief stimuli, returning to prestimulus behavior in less than 1 s . This requires a rapid rate of signal termination. The measured autodephosphorylation half-times of the chemotaxis RRs, however, vary from ∼4 s for CheY6-P to ∼4000 s for CheB1-P (Table 4). As R. sphaeroides does not have a CheZ homologue, an alternative dephosphorylation mechanism is required. Recently, CheA3 was shown to be a specific phosphatase for CheY6-P , but no phosphatases have been identified for the remaining chemotaxis RRs.
Phosphate sinks have been shown to be involved in signal termination in several bacterial signaling pathways –. To test whether a similar mechanism operates in R. sphaeroides, we used the model to predict the decay timecourse of RR-P levels resulting from simultaneously switching off autophosphorylation of CheA2 (reaction 1 in Table 1) and the phosphorylation of CheA3 by CheA4 (reaction 2 in Table 1). Although, the model incorporates the experimentally determined autodephosphorylation rates (reactions 10–15b of Table 1), interestingly, the model predicts that levels of all of the RR-Ps decay with half-lives shorter than ∼7 s (Table 4), which is much faster than their experimentally measured autodephosphorylation rates. Within the model, only CheY6-P has a phosphatase. The only route by which the model could predict dephosphorylation rates for the other RR-Ps that are faster than their autodephosphorylation rates is for one or more of the RRs to be acting as “phosphate sinks”, with the dephosphorylation of the target RR-P proceeding via reversed phosphotransfer to a CheA, which in turn transfers the phosphoryl group to the sink RR.
To determine which RRs could act as sinks, we simulated RR-P decay rates in cells deleted for a single RR e.g. for the cell lacking CheY3 we changed Y3T to zero and measured the simulation half-lives of the remaining RR-Ps. We found that only the removal of CheY6 greatly increased the simulation half-lives of the remaining RR-Ps (Table 4), suggesting that CheY6 acts as a phosphate sink for all of the other RR-Ps. Without CheY6, the simulation half-lives of the remaining RRs were in some cases (CheY3-P, CheY4-P and CheB2-P) increased beyond their autodephosphorylation half-times (Table 4). This is the result of significant quantities of CheA3-P and CheA2-P being present at steady state, and persisting for some time after the autophosphorylation reactions (reactions 1 and 2) were turned off. This allows levels of RR-P to be replenished resulting in a RR-P simulation half-time that is slower than their autodephosphorylation half-times. Interestingly, even in the absence of CheY6, the simulated dephosphorylation rate of CheB1-P was faster than its autodephosphorylation rate. In the absence of CheY6, the other RRs (CheY3, CheY4 and CheB2) may act as phosphate sinks for CheB1-P i.e. CheB1-P acts as a phosphodonor for CheA2 which in turn donates the phosphoryl groups to CheY3, CheY4 and CheB2. To test this we set the rate of phosphotransfer from CheB1-P to CheA2 (k−6) to zero and found that the simulated dephosphorylation half-time for CheB1-P was increased to 4295 s, which is comparable with its autodephosphorylation half-time indicating that in the absence of CheY6, one or more of other RRs therefore act as phosphate sinks for CheB1.
To confirm that the ability of CheY6 to act as a phosphate sink was robust to changes in parameters we performed a sensitivity analysis, where we varied each parameter by factors of 0.1, 0.5, 1.5 and 10, and measured the effect on the simulation half-life of CheB1-P (Table S1). For the parameters that were determined experimentally, the standard error lies well within the range covered by factors of 0.5 and 1.5. The simulation half-life of CheB1-P was robust to large changes in the majority of parameters, and in all cases remained much faster than the CheB1-P autodephosphorylation rate, but as would be expected showed some sensitivity towards those parameters directly involved in the operation of the CheY6 phosphate sink i.e. the rates of phosphotransfer between CheB1 and CheA2 and between CheA2 and CheY6. In addition, the system was also sensitive to large changes, well outside the range covered by experimental error in parameter determination, in the total concentrations of CheA2 and CheY6. This sensitivity analysis indicates that the parameter space in which the phosphate sink mechanism will work efficiently is broad and extends well beyond the range of experimental errors in the parameters themselves, suggesting that this pathway is likely to operate in vivo.
In summary, these simulated data suggest that not only is CheY6 a key regulator of flagellar motor rotation in R. sphaeroides, but it also acts as a “phosphate sink” ensuring rapid dephosphorylation of the other chemotaxis RRs (Figure 3A). This is very different from the S. meliloti sink where the sink CheY does not bind to the flagellar motor.
(A) The phosphotransfer reactions that allow CheY6 to work as a phosphate-sink for the other RR-Ps. CheY3-P, CheY4-P, CheB1-P can act as phosphodonors for CheA2. Phosphoryl groups can take either of two routes from CheA2 to the CheY6-phosphate-sink. CheA2-P can directly phosphorylate CheY6 (shown in green) or alternatively, can phosphorylate CheB2, which can transfer the phosphoryl group to CheA3 which then phosphorylates CheY6 (shown in blue). CheY6-P is rapidly dephosphorylated due to the specific phosphatase activity of the bifunctional enzyme CheA3. For diagrammatic simplicity, reversible reactions are shown as operating in the direction that leads towards the sink. (B) Diagram summarizing the role of CheB2 and CheA2 in relaying phosphoryl groups from CheA3-P to its non-cognate RRs, CheY3, CheY4 and CheB1. The reactions necessary for this phosphorelay are highlighted in red. At the cytoplasmic chemotaxis cluster, phosphoryl groups are transferred from CheA3-P to CheY6 and CheB2. CheB2-P then diffuses to the polar chemotaxis cluster where it serves as a phosphodonor for CheA2. CheA2-P subsequently acts as a phosphodonor for CheY3, CheY4 and CheB1. For diagrammatic simplicity, reactions which are reversible are shown as operating in the direction that leads towards the non-cognate RRs of CheA3.
The phosphatase activity of CheA3 is required for CheY6 to work as an efficient phosphate sink
In addition to containing the Hpt domain needed for phosphorylation of CheY6, CheA3 is also a phosphatase specific for CheY6-P. This phosphatase activity has previously been shown to be essential for chemotaxis . We used the model to determine the effect of phosphatase removal on RR-P levels and signal termination times, by setting the rate constants for the CheA3 phosphatase reactions (15a) and (15b) in Table 2 to zero. The model predicted very high steady state concentrations of all of the RR-Ps (Table 5), with phosphorylation levels of the total chemotaxis RR pool rising from ∼55% to ∼97%. This was the result of increased levels of CheY6-P (due to decreased dephosphorylation) leading to higher CheA2-P and CheA3-P concentrations and therefore higher levels of the other RR-Ps. The model also predicted that the signal termination times for all of the RR-Ps would be longer without the phosphatase (Table 4), as CheY6 would be less effective as a phosphate sink for the other RR-Ps. The model therefore highlights the importance of the phosphatase activity in CheA3, and demonstrates that although it is specific for CheY6-P, the phosphatase activity indirectly affects the concentration of the other RR-Ps and their signal termination rates as outlined above (Figure 3A). Removal of the phosphatase activity is therefore predicted to cause a general increase in RR-P levels, which could account for the non-chemotactic phenotype of the strains lacking phosphatase activity .
A phosphorelay pathway connects both chemotaxis clusters
We modeled the consequences of chemoeffector stimulation of either of the two chemotaxis clusters by either (i) turning off CheA2 autophosphorylation (reaction (1) – parameter k1 set to zero) to mimic attractant stimulation of the polar chemotaxis cluster or (ii) turning off the phosphorylation of CheA3 by CheA4 (reaction (2) – parameter k2 set to zero) to mimic attractant stimulation of the cytoplasmic chemotaxis cluster (Figure 4). As expected, when CheA2 autophosphorylation was turned off (case (i)) there was a reduction in the phosphorylation levels of each of the RRs (Figure 4) because CheA2-P serves as a phosphodonor for all of the RRs. However, counter-intuitively, significant levels of all RR-Ps remained, including CheY3-P, CheY4-P and CheB1-P, which can only be generated by CheA2-P.
Initially, CheA2 autophosphorylation in the polar cluster and the phosphorylation of CheA3 by CheA4 in the cytoplasmic cluster are occurring. To mimic attractant stimulation of the polar cluster, CheA2 autophosphorylation is turned off (k1 = 0) at the point labelled (A). This causes a drop in RR-P levels and a new steady state is reached. (B) Subsequently, CheA2 autophosphorylation is turned back on and the system returns to its original steady state. At point (C), the phosphorylation of CheA3 by CheA4 is turned off (k2 = 0) to mimic attractant stimulation of the cytoplasmic cluster. As a result of this, RR-P levels fall and a new steady state is reached. (D) Finally, phosphorylation of CheA3 by CheA4 is turned back on and the system returns to its initial steady state.
Analysis of the modeling results from case (i) revealed that even though CheA2 autophosphorylation had been turned off, significant levels of CheA2-P were present and were being generated by the reversal of reaction (7) (Table 1) i.e. CheB2-P was acting as a phosphodonor for CheA2 (as demonstrated in Figure 2C). In this case, CheY6 and CheB2 were phosphorylated by CheA3-P; CheB2-P then served as a phosphodonor for CheA2 i.e. CheB2 transfers phosphoryl groups between CheA3-P and CheA2. The CheA2-P generated in this way could then phosphorylate CheY3, CheY4 and CheB1. This result suggests that CheA3-P is linked to the RRs, CheY3, CheY4 and CheB1, via a multistep phosphorelay i.e. CheA3-P (His) to CheB2 (Asp) to CheA2 (His) to CheY3/CheY4/CheB1 (Asp).
In case (ii), switching off the phosphorylation of CheA3 by CheA4 caused a reduction not only in the levels of CheY6-P and CheB2-P, but also in levels of CheY3-P, CheY4-P and CheB1-P. Levels of CheY3-P, CheY4-P and CheB1-P were affected because (a) they were dephosphorylated faster since the reduction in CheY6-P levels was accompanied by an increase in the unphosphorylated CheY6 levels which acts as a phosphate sink and (b) there was no input of phosphoryl groups at the cytoplasmic cluster for CheB2 to transfer to these RRs via CheA2. These results indicate that even when CheA2 autophosphorylation is occurring, the bifunctional kinase/phosphatase in the cytoplasmic chemotaxis cluster makes a significant contribution to the phosphorylation levels of all of the RRs.
We performed a sensitivity analysis to look at the effect of varying each of the model parameters on levels of CheY4-P when CheA2 autophosphorylation is turned off; under these conditions CheY4-P levels give a measure of the extent to which the phosphorelay is occurring (Table S2). The system was robust to changes in many of the parameters although as would be expected was sensitive to changes in parameters that directly affect either i) the rate of entry or exit of phosphoryl groups from the system e.g. rate of phosphorylation of CheA3 by CheA4, rate of CheY6-P dephosphorylation (autodephosphorylation and phosphatase assisted), and the expression levels of CheA3 and CheY6 or ii) the functioning of the phosphorelay e.g. the expression levels of CheA2 and CheB2, rates of phosphotransfer between CheA3 and CheB2, between CheB2 and CheA2, and between CheA2 and CheY4. However, despite this sensitivity in almost all cases at least some phosphorylation of CheY4 was predicted indicating that the phosphorelay remained operational. In the two remaining extreme cases, where CheY6 expression levels were ten times higher than usual or where the rate of phosphorylation of CheA3 by CheA4 was ten-fold lower than the measured rate, levels of all RR-Ps, not just CheY4-P, were extremely low. These results indicate that the phosphorelay operates over a broad range of parameter space, although the extent to which it operates is sensitive to large changes in some of the parameters.
The experimental work leading up to this study produced an outline architecture of the complex signaling network controlling R. sphaeroides chemotaxis . However, the mechanism of integrating the signals produced by each of the signaling clusters to control the flagellar motor was unclear. Mathematical modeling has provided considerable insight into the probable functioning of simpler chemotaxis pathways , , , and a control engineering approach has recently been used in R. sphaeroides to discriminate between several possible mechanisms of CheY control of the flagellar motor . In this study, a mathematical model of R. sphaeroides chemotaxis was formulated that integrates in vivo and in vitro biochemical data on the kinetic preferences of the signaling reactions with in vivo measurements of protein copy number. Analysis of the model revealed two interesting features of the signaling network, both of which rely on reversed phosphotransfer from RR-Ps to CheA. Firstly, rapid signal termination for all chemotaxis RR-Ps may be achieved by CheY6 acting as a phosphate sink in addition to being the primary motor control protein (Figure 3A). Secondly, a novel phosphorelay involving CheB2 appears to link the cytoplasmic and polar chemotaxis clusters (Figure 3B). Together these two network features provide the bifunctional kinase/phosphatase, CheA3, with the means to increase or decrease the concentration of all of the chemotaxis RR-Ps and therefore to regulate the output of the two chemosensory clusters.
CheY6 is a phosphate sink for all of the chemotaxis RR-Ps
Phosphate sinks provide an alternative mechanism for dephosphorylating RR-Ps , , instead of simply hydrolyzing the phosphoryl group (as in autodephosphorylation or phosphatase-assisted-dephosphorylation), the phosphoryl group is transferred to a HPK, which subsequently transfers it to the “phosphate sink” RR. The phosphoryl group is then hydrolyzed from the “phosphate sink” by either autodephosphorylation or phosphatase-assisted-dephosphorylation. The model presented in this study predicted that signal termination occurs rapidly in R. sphaeroides, with all RR-Ps dephosphorylating with half-times of less than ∼7 s (Table 4). This is consistent with the observed stimulus response time of 1 s for R. sphaeroides , since with a decay half-time of ∼7 s, CheY-P levels could fall by ∼10% during 1s, which, assuming that the R. sphaeroides motor is as ultrasensitive to changes in CheY-P levels as the E. coli motor , would be sufficient to give a significant change in motor rotation bias.
Prior to this study, it was known that CheY6-P with the aid of its specific phosphatase, the bifunctional protein CheA3, could dephosphorylate rapidly , however, the other RR-Ps were known to autodephosphorylate with half-times in excess of 36 s, with CheB1-P taking over 4000 s. By removing each of the RRs in turn from the model, we found that CheY6 was acting as a “phosphate sink” for the other RR-Ps, since cells lacking CheY6 showed much slower dephosphorylation rates for the remaining RR-Ps (Table 4 and Figure 3A). Furthermore, we showed that removal of the phosphatase activity of CheA3 from the model increased the dephosphorylation half-times of all of the RR-Ps, indicating that the phosphatase activity is required for efficient operation of the CheY6 phosphate sink and rapid signal termination. This phosphate sink role for CheY6 is additional to its primary role as a direct regulator of flagellar rotation .
CheY6 differs in several ways from the prototypical phosphate sink, CheY1 from S. meliloti . CheY6 directly controls flagellar motor rotation by binding FliM , , and has a dedicated phosphatase, in contrast, S. meliloti CheY1 does not bind FliM and appears to function only as a “phosphate sink”. Another fundamental difference is the rate of dephosphorylation; CheY6-P dephosphorylates much faster than the autodephosphorylation rates of the RRs for which it acts as a sink whereas S. meliloti CheY1-P does not autodephosphorylate any faster than the motor binding RR, CheY2-P, for which it is a sink. The S. meliloti sink does not need to dephosphorylate quickly because it does not directly affect flagellar rotation and so phosphoryl groups can be stored on it until autodephosphorylation occurs, in contrast, R. sphaeroides CheY6 is a key regulator of flagellar rotation and therefore requires rapid signal termination.
A CheB2 mediated phosphorelay connects the polar and cytoplasmic signaling clusters
As part of our interrogation of the model, we simulated attractant stimulation of the polar chemotaxis cluster by turning off autophosphorylation of CheA2, while allowing phosphorylation of CheA3 by CheA4 to occur (Figure 4). Interestingly under these conditions, even though CheA3-P cannot directly phosphorylate CheY3, CheY4, and CheB1, the model predicted non-zero concentrations of these RR-Ps. This is the result of the action of a phosphorelay where phosphoryl groups from CheA3-P (His) are transferred to CheB2 (Asp) then to CheA2 (His) and subsequently to either CheY3, CheY4 or CheB1 (Asp) (Figure 3B). Direct testing of the in vivo importance of this phosphorelay is confounded by the dual role of CheB2, firstly as a chemoreceptor methylesterase and secondly as a potential intermediate in the phosphorelay. The methylesterase activity of CheB2 is required for normal chemotaxis and it is not possible to block the phosphorylation of CheB2 by mutagenesis without impairing the control of this methylesterase activity. It is therefore not known the extent to which this CheB2 mediated phosphorelay operates in vivo; however, the model does incorporate both in vitro kinetic preference data and in vivo protein expression levels, and this suggests that the phosphorelay may operate in vivo, allowing the cytoplasmic cluster to make a significant contribution to phosphorylation levels of the non-cognate RRs; CheY3, CheY4 and CheB1.
The model in this study does not include adaptation as this is a poorly understood process in R. sphaeroides, with little experimental data. However, it is possible that the adaptation pathway could act to reduce the elevated RR-P levels caused by a constant influx of phosphoryl groups to the polar cluster from the cytoplasmic cluster by modifying the polar receptors in such a way as to reduce the autophosphorylation rate of the polar kinase, CheA2 i.e. the cell could adapt to constant signals from the cytoplasmic cluster. Although when cells are performing chemotaxis and swimming through gradients of chemoeffector, signals from the cytoplasmic cluster will vary over time and will make a significant contribution to RR-P levels. The relative contribution of this phosphorelay to levels of CheY3-P, CheY4-P and CheB1-P will be modulated by signals coming through the transmembrane chemoreceptors that directly control the rate of CheA2 autophosphorylation and would be greatest when the autophosphorylation rate of CheA2 is low and the rate of phosphorylation of CheA3 by CheA4 is high. These conditions could arise when cells are swimming up a gradient of a specific attractant which is sensed by the transmembrane chemoreceptors, while the metabolic state of the cell is worsening due to, for example, decreasing concentrations of an essential nutrient (for which there may not be a transmembrane chemoreceptor). Under such conditions, the increased rate of phosphorylation of CheA3 by CheA4, coupled with the CheB2/CheA2 mediated phosphorelay, could raise levels CheY3-P, CheY4-P and CheY6-P, allowing cells to override their favourable response to the extracellular attractant and swim away from these unfavourable environments.
Numerous examples of other two-component systems employing phosphorelays have been described –; however, to the best of our knowledge this is the first example of a phosphorelay involving two distinct HPKs localized to different regions of the cell, and also, the first phosphorelay to be found in a chemotaxis signaling pathway. Given that over 50% of bacteria with any che genes have more than two cheAs , , , it seems likely that phosphorelays allowing communication between different CheA homologues could be involved in chemotactic signaling in a wide range of bacterial species.
Signal integration by the cytoplasmic cluster
The polar cluster senses extracellular signals while the cytoplasmic cluster is believed to sense the metabolic state of the cell . The concentration of each RR-P depends not only on polar kinase activity but also on the balance of kinase and phosphatase activity in the cytoplasmic cluster. The kinase activity of the cytoplasmic cluster resides in CheA4 and the phosphatase activity resides in CheA3; both proteins have P5 (regulatory) domains and it is therefore likely that both activities will be regulated by environmental stimuli , . A stimulus that increases phosphatase activity would have the effect of reducing levels of all RR-Ps, since the action of the phosphatase would directly accelerate CheY6-P dephosphorylation leaving more unphosphorylated CheY6 to function as a phosphate sink for the other RR-Ps. Such a mechanism could allow the cytoplasmic cluster to tune or modulate signals coming from the polar cluster since increased phosphatase activity would lead to a general decrease in chemotaxis RR-P levels. In contrast, a stimulus that increased kinase activity at the cytoplasmic cluster would increase levels of all RR-Ps because CheA3-P would phosphorylate CheY6 and CheB2 directly; CheB2 would then shuttle the phosphoryl groups to CheA2 and from there onto the other RRs while phosphorylation of CheY6 would reduce its capacity as a phosphate sink resulting in a general increase in RR-P levels. Therefore the overall sensory output of the pathway depends critically on the relative activity of CheA3 and CheA4, and potentially provides a mechanism for signals about the metabolic state of the cell to modulate signals regarding the extracellular environment.
Materials and Methods
Full details on the mathematical model are included in Text S1. Briefly, the law of mass action was applied to the reactions detailed in Table 1 to produce a system of non-linear ordinary differential equations (ODEs), which were solved using Matlab (MathWorks). The model was parameterized with data from the literature , , , , – and our own experiments as detailed in Tables 2&3. A parameter fit of the phosphotransfer rates between each kinase and RR (time course data) with that of a mathematical model describing the in vitro reactions was performed. A number of local, global and genetic algorithm optimisation procedures were employed (simulated annealing, Hooke and Jeeves, least squares, Levenberg-Marquardt, Nelder-Mead, steepest descent and the genetic algorithm) to obtain a robust set of parameters (Table 3).
Plasmids and strains
The plasmids and strains used are shown in Table S3. E. coli strains were grown in LB medium at 37°C. Where required, antibiotics were used at concentrations of 100 µg ml−1 for ampicillin and 25 µg ml−1 for kanamycin.
His-tagged and GST-tagged R. sphaeroides CheA, CheY and CheB proteins were purified as described previously . Protein purity and concentration was measured as described . Purified proteins were stored at −20°C.
Preparation of CheA3P1-32P
CheA3P1 was phosphorylated using [γ-32P] ATP and CheA4, and purified as described previously . The final preparation of CheA3P1-32P was free of ATP and CheA4.
Detection of phosphotransfer from the response regulators to CheA2
Assays were performed at 20°C in TGMNKD buffer (50 mM Tris HCl, 10% (v/v) glycerol, 5 mM MgCl2, 150 mM NaCl, 50 mM KCl, 1 mM DTT, pH 8.0). CheA3P1-32P was used to phosphorylate the RRs, CheY6 and CheB2, in these assays because it is a good phosphodonor for these proteins and even after prolonged incubation (>1 hour) CheA3P1-32P does not act as a direct phosphodonor for CheA2 (Figure 3A); therefore any CheA2-P generated in these assays is due to phosphotransfer from RR-P to CheA2 rather than direct phosphotransfer from CheA3P1-P to CheA2. 30 µM CheA3P1-32P was mixed with 5 µM CheA2 prior to the addition of 10 µM RR. Following the addition of RR, reaction aliquots of 10 µl were taken at the indicated timepoints and quenched immediately in 5 µl of 3 X SDS-PAGE loading dye (7.5% (w/v) SDS, 90 mM EDTA, 37.5 mM Tris HCl, 37.5% glycerol, 3% (v/v) β-mercaptoethanol, pH 6.8). Quenched samples were analyzed using SDS-PAGE and phosphorimaging as described previously.
Protein expression levels
The effect of parameter variation on the simulation half-life of CheB1-P.
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The effect of parameter variation on the predicted levels of CheY4-P when CheA2 autophosphorylation is turned off (k1 = 0).
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Plasmids and bacterial strains used in this study.
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Conceived and designed the experiments: MJT SLP PKM JPA. Performed the experiments: SLP. Analyzed the data: MJT SLP. Contributed reagents/materials/analysis tools: MJT SLP. Wrote the paper: MJT SLP PKM JPA.
- 1. Stock AM, Robinson VL, Goudreau PN (2000) Two-component signal transduction. Annu Rev Biochem 69: 183–215.
- 2. Bray D, Levin MD, Morton FC (1998) Receptor clustering as a cellular mechanism to control sensitivity. Nature 393: 85–88.
- 3. Tindall MJ, Maini PK, Porter SL, Armitage JP (2008) Overview of mathematical approaches used to model bacterial chemotaxis II: bacterial populations. Bull Math Biol 70: 1570–1607.
- 4. Tindall MJ, Porter SL, Maini PK, Gaglia G, Armitage JP (2008) Overview of mathematical approaches used to model bacterial chemotaxis I: the single cell. Bull Math Biol 70: 1525–1569.
- 5. Hansen CH, Endres RG, Wingreen NS (2008) Chemotaxis in Escherichia coli: a molecular model for robust precise adaptation. PLoS Comput Biol 4: e1.
- 6. Tu Y, Shimizu TS, Berg HC (2008) Modeling the chemotactic response of Escherichia coli to time-varying stimuli. Proc Natl Acad Sci USA 105: 14855–14860.
- 7. Endres RG, Oleksiuk O, Hansen CH, Meir Y, Sourjik V, et al. (2008) Variable sizes of Escherichia coli chemoreceptor signaling teams. Mol Syst Biol 4: 211.
- 8. Goldman JP, Levin MD, Bray D (2009) Signal amplification in a lattice of coupled protein kinases. Mol BioSyst 5: 1853–1859.
- 9. Rao CV, Kirby JR, Arkin AP (2004) Design and diversity in bacterial chemotaxis: a comparative study in Escherichia coli and Bacillus subtilis. PLoS Biol 2: e49.
- 10. Alon U, Surette MG, Barkai N, Leibler S (1999) Robustness in bacterial chemotaxis. Nature 397: 168–171.
- 11. Hazelbauer GL, Falke JJ, Parkinson JS (2008) Bacterial chemoreceptors: high-performance signaling in networked arrays. Trends Biochem Sci 33: 9–19.
- 12. Wadhams GH, Armitage JP (2004) Making sense of it all: Bacterial chemotaxis. Nat Rev Mol Cell Bio 5: 1024–1037.
- 13. Szurmant H, Ordal GW (2004) Diversity in chemotaxis mechanisms among the Bacteria and Archaea. Microbiol Mol Biol Rev 68: 301–319.
- 14. Maddock JR, Shapiro L (1993) Polar location of the chemoreceptor complex in the Escherichia coli cell. Science 259: 1717–1723.
- 15. Greenfield D, McEvoy AL, Shroff H, Crooks GE, Wingreen NS, et al. (2009) Self-organization of the Escherichia coli chemotaxis network imaged with super-resolution light microscopy. PLoS Biol 7: e1000137.
- 16. Briegel A, Ortega DR, Tocheva EI, Wuichet K, Li Z, et al. (2009) Universal architecture of bacterial chemoreceptor arrays. Proc Natl Acad Sci USA 106: 17181–17186.
- 17. Borkovich KA, Kaplan N, Hess JF, Simon MI (1989) Transmembrane signal transduction in bacterial chemotaxis involves ligand-dependent activation of phosphate group transfer. Proc Natl Acad Sci USA 86: 1208–1212.
- 18. Ninfa EG, Stock A, Mowbray S, Stock J (1991) Reconstruction of the bacterial chemotaxis signal transduction system from purified components. J Biol Chem 266: 9764–9770.
- 19. Boldog T, Grimme S, Li M, Sligar SG, Hazelbauer GL (2006) Nanodiscs separate chemoreceptor oligomeric states and reveal their signaling properties. Proc Natl Acad Sci USA 103: 11509–11514.
- 20. Hess JF, Bourret RB, Simon MI (1988) Histidine phosphorylation and phosphoryl group transfer in bacterial chemotaxis. Nature 336: 139–143.
- 21. Sanders DA, Gillece-Castro BL, Stock AM, Burlingame AL, Koshland DE Jr (1989) Identification of the site of phosphorylation of the chemotaxis response regulator protein, CheY. J Biol Chem 264: 21770–21778.
- 22. Bourret RB, Hess JF, Simon MI (1990) Conserved aspartate residues and phosphorylation in signal transduction by the chemotaxis protein CheY. Proc Natl Acad Sci USA 87: 41–45.
- 23. Welch M, Oosawa K, Aizawa S-I, Eisenbach M (1993) Phosphorylation-dependent binding of a signal molecule to the flagellar switch of bacteria. Proc Natl Acad Sci USA 90: 8787–8791.
- 24. Dyer CM, Vartanian AS, Zhou H, Dahlquist FW (2009) A Molecular Mechanism of Bacterial Flagellar Motor Switching. J Mol Biol 388: 71–84.
- 25. Lupas A, Stock J (1989) Phosphorylation of an N-terminal regulatory domain activates the CheB methylesterase in bacterial chemotaxis. J Biol Chem 264: 17337–17342.
- 26. Sourjik V, Berg HC (2002) Receptor sensitivity in bacterial chemotaxis. Proc Natl Acad Sci USA 99: 123–127.
- 27. Thomas SA, Brewster JA, Bourret RB (2008) Two variable active site residues modulate response regulator phosphoryl group stability. Mol Microbiol 69: 453–465.
- 28. Hess JF, Oosawa K, Kaplan N, Simon MI (1988) Phosphorylation of three proteins in the signalling pathway of bacterial chemotaxis. Cell 53: 79–87.
- 29. Silversmith RE, Levin MD, Schilling E, Bourret RB (2008) Kinetic characterization of catalysis by the chemotaxis phosphatase CheZ: modulation of activity by the phosphorylated CheY substrate. J Biol Chem 283: 756–765.
- 30. Porter SL, Wadhams GH, Armitage JP (2008) Rhodobacter sphaeroides: Complexity in chemotactic signalling. Trends Microbiol 16: 251–260.
- 31. Hamer R, Chen P-Y, Armitage JP, Reinert G, Deane CM (2010) Deciphering chemotaxis pathways using cross species comparisons. BMC Syst Biol 4: 3.
- 32. Wuichet K, Zhulin IB (2010) Origins and diversification of a complex signal transduction system in prokaryotes. Sci Signal 3: ra50.
- 33. Armitage JP, Macnab RM (1987) Unidirectional intermittent rotation of the flagellum of Rhodobacter sphaeroides. J Bacteriol 169: 514–518.
- 34. Porter SL, Warren AV, Martin AC, Armitage JP (2002) The third chemotaxis locus of Rhodobacter sphaeroides is essential for chemotaxis. Mol Microbiol 46: 1081–1094.
- 35. Martin AC, Wadhams GH, Armitage JP (2001) The roles of the multiple CheW and CheA homologues in chemotaxis and in chemoreceptor localization in Rhodobacter sphaeroides. Mol Microbiol 40: 1261–1272.
- 36. Pilizota T, Brown MT, Leake MC, Branch RW, Berry RM, et al. (2009) A molecular brake, not a clutch, stops the Rhodobacter sphaeroides flagellar motor. Proc Natl Acad Sci USA 106: 11582–11587.
- 37. Poggio S, breu-Goodger C, Fabela S, Osorio A, Dreyfus G, et al. (2007) A complete set of flagellar genes acquired by horizontal transfer coexists with the endogenous flagellar system in Rhodobacter sphaeroides. J Bacteriol 189: 3208–3216.
- 38. del Campo AM, Ballado T, de la Mora J, Poggio S, Camarena L, et al. (2007) Chemotactic control of the two flagellar systems of Rhodobacter sphaeroides is mediated by different sets of CheY and FliM proteins. J Bacteriol 189: 8397–8401.
- 39. Porter SL, Wadhams GH, Martin AC, Byles ED, Lancaster DE, et al. (2006) The CheYs of Rhodobacter sphaeroides. J Biol Chem 281: 32694–32704.
- 40. Martin AC, Wadhams GH, Shah DSH, Porter SL, Mantotta JC, et al. (2001) CheR- and CheB-dependent chemosensory adaptation system of Rhodobacter sphaeroides. J Bacteriol 183: 7135–7144.
- 41. Shah DSH, Porter SL, Martin AC, Hamblin PA, Armitage JP (2000) Fine tuning bacterial chemotaxis: analysis of Rhodobacter sphaeroides behaviour under aerobic and anaerobic conditions by mutation of the major chemotaxis operons and cheY genes. EMBO J 19: 4601–4613.
- 42. Shah DS, Porter SL, Harris DC, Wadhams GH, Hamblin PA, et al. (2000) Identification of a fourth cheY gene in Rhodobacter sphaeroides and interspecies interaction within the bacterial chemotaxis signal transduction pathway. Mol Microbiol 35: 101–112.
- 43. Porter SL, Armitage JP (2004) Chemotaxis in Rhodobacter sphaeroides requires an atypical histidine protein kinase. J Biol Chem 279: 54573–54580.
- 44. Wadhams GH, Warren AV, Martin AC, Armitage JP (2003) Targeting of two signal transduction pathways to different regions of the bacterial cell. Mol Microbiol 50: 763–770.
- 45. Porter SL, Armitage JP (2002) Phosphotransfer in Rhodobacter sphaeroides chemotaxis. J Mol Biol 324: 35–45.
- 46. Wadhams GH, Martin AC, Porter SL, Maddock JR, Mantotta JC, et al. (2002) TlpC, a novel chemotaxis protein in Rhodobacter sphaeroides, localizes to a discrete region in the cytoplasm. Mol Microbiol 46: 1211–1221.
- 47. Bell CH, Porter SL, Strawson A, Stuart DI, Armitage JP (2010) Using structural information to change the phosphotransfer specificity of a two-component chemotaxis signalling complex. PLoS Biol 8: e1000306.
- 48. Porter SL, Roberts MAJ, Manning CS, Armitage JP (2008) A bifunctional kinase-phosphatase in bacterial chemotaxis. Proc Natl Acad Sci USA 105: 18531–18536.
- 49. Ferre A, de la Mora J, Ballado T, Camarena L, Dreyfus G (2004) Biochemical study of multiple CheY response regulators of the chemotactic pathway of Rhodobacter sphaeroides. J Bacteriol 186: 5172–5177.
- 50. Berry RM, Armitage JP (2000) Response kinetics of tethered Rhodobacter sphaeroides to changes in light intensity. Biophys J 78: 1207–1215.
- 51. Sourjik V, Schmitt R (1998) Phosphotransfer between CheA, CheY1, and CheY2 in the chemotaxis signal transduction chain of Rhizobium meliloti. Biochemistry 37: 2327–2335.
- 52. Jimenez-Pearson MA, Delany I, Scarlato V, Beier D (2005) Phosphate flow in the chemotactic response system of Helicobacter pylori. Microbiology 151: 3299–3311.
- 53. Rasmussen AA, Porter SL, Armitage JP, Sogaard-Andersen L (2005) Coupling of multicellular morphogenesis and cellular differentiation by an unusual hybrid histidine protein kinase in Myxococcus xanthus. Mol Microbiol 56: 1358–1372.
- 54. Rasmussen AA, Wegener-Feldbrugge S, Porter SL, Armitage JP, Sogaard-Andersen L (2006) Four signalling domains in the hybrid histidine protein kinase RodK of Myxococcus xanthus are required for activity. Mol Microbiol 60: 525–534.
- 55. Tindall MJ, Porter SL, Wadhams GH, Maini PK, Armitage JP (2009) Spatiotemporal modelling of CheY complexes in Escherichia coli chemotaxis. Prog Biophys Mol Biol 100: 40–46.
- 56. Roberts M, August E, Hamadeh A, Maini P, McSharry P, et al. (2009) A model invalidation-based approach for elucidating biological signalling pathways, applied to the chemotaxis pathway in R. sphaeroides. BMC Syst Biol 3: 105.
- 57. Cluzel P, Surette M, Leibler S (2000) An ultrasensitive bacterial motor revealed by monitoring signaling proteins in single cells. Science 287: 1652–1655.
- 58. Mitrophanov AY, Groisman EA (2008) Signal integration in bacterial two-component regulatory systems. Genes Dev 22: 2601–2611.
- 59. Perego M, Hanstein C, Welsh KM, Djavakhishvili T, Glaser P, et al. (1994) Multiple protein-aspartate phosphatases provide a mechanism for the integration of diverse signals in the control of development in B. subtilis. Cell 79: 1047–1055.
- 60. Ogino T, Matsubara M, Kato N, Nakamura Y, Mizuno T (1998) An Escherichia coli protein that exhibits phosphohistidine phosphatase activity towards the HPt domain of the ArcB sensor involved in the multistep His-Asp phosphorelay. Mol Microbiol 27: 573–585.
- 61. Appleby JL, Parkinson JS, Bourret RB (1996) Signal transduction via the multi-step phosphorelay: not necessarily a road less traveled. Cell 86: 845–848.
- 62. Scott KA, Porter SL, Bagg EAL, Hamer R, Hill JL, et al. (2010) Specificity of localization and phosphotransfer in the CheA proteins of Rhodobacter sphaeroides. Mol Microbiol 76: 318–330.
- 63. Slovak PM, Porter SL, Armitage JP (2006) Differential localization of Mre proteins with PBP2 in Rhodobacter sphaeroides. J Bacteriol 188: 1691–1700.
- 64. Slovak PM, Wadhams GH, Armitage JP (2005) Localization of MreB in Rhodobacter sphaeroides under conditions causing changes in cell shape and membrane structure. J Bacteriol 187: 54–64.
- 65. Ind AC, Porter SL, Brown MT, Byles ED, de Beyer JA, et al. (2009) An inducible expression plasmid for Rhodobacter sphaeroides and Paracoccus denitrificans. Appl Environ Microbiol 75: 6613–6615.
- 66. Porter SL, Wadhams GH, Armitage JP (2007) In vivo and in vitro analysis of the Rhodobacter sphaeroides chemotaxis signaling complexes. Method Enzymol 423: 392–413.
- 67. Ben-Anat Porat Y, Zan-Bar I, Ravid A (1995) Quantitative dot-blot assay for low titer anti-lipopolysaccharide antibodies in human plasma. J Immunol Methods 180: 213–218.
- 68. Brown MT (2009) Control of the unidirectional motor in Rhodobacter sphaeroides. D. Phil. Thesis. University of Oxford.
- 69. Gould , Marcus (2006) Chemotaxis gene expression in Rhodobacter sphaeroides WS8N. D. Phil. Thesis. University of Oxford.