- Research article
- Open Access
Understanding system dynamics of an adaptive enzyme network from globally profiled kinetic parameters
BMC Systems Biology volume 8, Article number: 4 (2014)
A major challenge in mathematical modeling of biological systems is to determine how model parameters contribute to systems dynamics. As biological processes are often complex in nature, it is desirable to address this issue using a systematic approach. Here, we propose a simple methodology that first performs an enrichment test to find patterns in the values of globally profiled kinetic parameters with which a model can produce the required system dynamics; this is then followed by a statistical test to elucidate the association between individual parameters and different parts of the system’s dynamics.
We demonstrate our methodology on a prototype biological system of perfect adaptation dynamics, namely the chemotaxis model for Escherichia coli. Our results agreed well with those derived from experimental data and theoretical studies in the literature. Using this model system, we showed that there are motifs in kinetic parameters and that these motifs are governed by constraints of the specified system dynamics.
A systematic approach based on enrichment statistical tests has been developed to elucidate the relationships between model parameters and the roles they play in affecting system dynamics of a prototype biological network. The proposed approach is generally applicable and therefore can find wide use in systems biology modeling research.
Systems biology aims to unravel the design principles of living organisms from a network perspective [1, 2]. Advances in experimental studies have generated a large amount of data on several key biological processes [3–8], and networks of interactions between molecular species have been hypothesized [9–14]. Despite these advances, one unresolved challenge in systems biology is to understand how the hypothesized molecular interactions can lead to the observed biological phenomenon for complex biological systems. One way of pursuing this is via mathematical modeling of biological processes, which can also generate testable hypothesis for future experiments.
Biological processes are often complicated, and the complexity of their mathematical models usually increases with the amount of parameters involved. This generally gives rise to two fundamental problems in mathematical modeling. First, it is possible to have multiple sets of parameter values that are equally likely to produce the observed data and finding the “best” parameter set might be insufficient to fully characterize a biological system if such a parameter set is not the only set with biological relevance . Second, understanding the role of individual parameters on different aspects of observed systems dynamics can be difficult for parameter-rich models as it might be too time consuming to explore this systematically and exhaustively. Although a number of approaches, for instance the genetic algorithm-based method  and others [15, 17], have been developed to search for parameter solutions in high dimensional spaces, they have not been extended to make inferences on the contribution of individual parameters to specific components of the system dynamics. As such, in this paper we propose a general framework for addressing the aforementioned problems in mathematical modeling of biological systems. Our methodology can be summarized as follows. For a given mathematical model of a biological process, one first defines the system’s dynamics that the model is required to reproduce; one then searches through the parameter space by a sampling method, and keeps those sets of parameters with which the model can produce the required dynamics. These then form a matrix Z of functional parameter values, with each element z ij denoting the value of the j- th parameter in the i-th parameter set. This matrix then undergoes statistical analysis to test whether a particular parameter is biased towards a certain value (or certain range of values) for the model to produce the target dynamics. After this is done for all parameters, the results can be compiled to identify recurrent parameter values and any patterns they might form. Finally, if the system’s dynamics can be decomposed into different components or parts, then further analysis can be performed to associate a parameter with a particular aspect of the dynamics.
Our methodology is demonstrated on a well-studied example of adaptation dynamics, that of the chemotaxis of Escherichia coli[18–21]. Generally speaking, adaptation refers to the ability of an organism adjusting to a new environment, and it is thought to be an important attribute for survival under fluctuating conditions [22–28]. In Escherichia coli, adaptation allows its chemotaxis system to reset stimulus-induced output to pre-stimulus value, even upon persistent external stimulation [29, 30]. The dynamics of chemotaxis adaptation has two parts (Figure 1A): first, the output signal of the system exhibits a sharp increase after the initial stimulation, and this is referred to as the sensitivity phase; second, after the initial sharp rise, the output signal decays to its initial state, and this is referred to as the precision phase. Figure 1B illustrates the molecular processes involved, which have been identified experimentally [31, 32]. Briefly, input signals are fed into the histidine kinase CheA-chemoreceptor R complex, and CheA then phosphorylates CheY (which can be dephosphorylated by CheZ) to regulate the process that drives the flagella of a bacteria. The key point here is that the activity of CheA is determined by the level of methylation of the CheA-bound receptor complex, which is controlled by demethylase CheB, which is in turn positively regulated by CheA itself, forming a negative feedback loop (Figure 1B). Recently, Ma et al.  constructed a mathematical model for a three-node enzyme network and found that only two major types of network topologies can produce dynamics associated with adaptation (Figure 1C and Additional file 1: Figure S8). One topology consists of a negative feed-back loop with a buffer node (NFBLB for short): node A positively influences the production of nodes B and C, and node B in return negatively regulates node A (Figure 1C). The other topology has an incoherent feed-forward loop with a proportioner node (IFFLP for short): here, node A induces node B, which in turn induces node C, and nodes A, B and C also have inhibiting role on nodes C, A and B, respectively (Additional file 1: Figure S8). The enzyme network driving the chemotaxis of E. coli has been found to resemble the NFBLB model . Thus, in the rest of this paper, we use the NFBLB model to demonstrate our methodology in order to better understand how individual parameters contribute to the mechanism underlying the chemotaxis of E. coli. Empirical findings from the literature will be compared to our numerical results for validation purposes. Results for the IFFLP model will be presented in supplemental data.
Model of the adaptive enzyme network
The original E. coli chemotaxis model was proposed as a two-state model  and was later expanded to include the phosphorylation cascade . In this study, the model we used is essentially the same as that used by  and , in which we consider the CheA-bound receptor complex as a single entity (node A in Figure 1C) and assume that this receptor complex exists in either a CheA active (A m) or a CheA inactive (A) state. The superscript m denotes the methylated form of the receptor complex.
The binding kinetic equation for the inactive receptor complex is given by,
where I denotes the concentration of chemo-attractant, K IA is the ligand dissociation constant and k IA is the ligand catalytic constant.
The demethylation kinetic equation for the active receptor complex is given by,
where B P denotes the concentration of phosphorylated demethylase CheB, K BA is the dissociation constant of phosphorylated CheB and k BA is the catalytic constant of phosphorylated CheB.
The process of phosphate group transfer from active CheA to CheB is given by,
where K AB and k AB are the dissociation constant and the catalytic constant of active CheA, respectively.
The dephosphorylation of phosphorylated CheB is given by,
where k FBB is the dephosphorylation constant.
Transfer of the phosphate group from active CheA to CheY (node C in Figure 1C) is given by,
where K AC and k AC are the dissociation constant and the catalytic constant of active CheA, respectively.
The dephosphorylation of phosphorylated CheY by CheZ (represented by F C in Figure 1C and by Z in the equation below) is given by,
where K ZC and k ZC are the dissociation constant and the catalytic constant of CheZ, respectively.
where I denotes the input signal (i.e. the concentration of chemo-attractant); A, B and C denote the concentrations in active states; (1-A), (1-B) and (1-C) denote the concentrations in inactive forms; F B and F C are the concentration of deactivating enzymes (assumed to be a constant value of 0.5 as in ) that transform the active states of B and C into inactive states. Kinetic parameters k ij and K ij are respectively the catalytic rate constant and Michaelis-Menten constant for the catalytic reaction between substrate i and its regulator (activating or deactivating) enzyme j, where i and j = A, B, C, F B , or F C . Note that for each node A, B or C, the first term (v 1 ) and the second term (v 2 ) of the equation represent its activation and deactivation rates respectively.
Two quantities were used to evaluate the performance of a kinetic parameter set in producing adaptation dynamics: (i) sensitivity to the input stimulus (equation (8)), which is defined as the difference between output response and the initial steady-state value, and (ii) precision (equation (9)), which is defined as the inverse of the difference between pre- and post-stimulus steady state values. The corresponding mathematical equations for these two quantities are :
where O1 and O2 represent two steady-state values, respectively corresponding to the two input values I1 and I2 (I1 = 0.5 and I2 =0.6 following ), and Op is the peak value of a transient pulse in response to the input change (see Figure 1A).
Sampling parameter values and numerical simulations
As in , Latin hypercube sampling  was used to sample uniformly at random the values of kinetic parameters on a logarithmic scale, with the catalytic rate constant k being in the range of [10-1, 101] and the Michaelis-Menten constant K in the range of [10-3, 102]. These two parameter ranges were chosen by Ma et al.  to, presumably, minimize computational cost while covering previously reported values used to model the E coli chemotaxis system [36–38]. In order for our results to be comparable with those from previous studies, we opted to use the same parameter ranges in this paper. For each parameter set, the model (equation (7) for the NFBLB model and equation (S1) in the supplemental data for the IFFLP model) was numerically simulated and those producing the desired adaptation dynamics were identified. The original 104 parameter sets sampled by Ma et al. for the NFBLB model produced only eight kinetic solutions , which are insufficient for discovering parameter motifs with any statistical significance. To remedy this, a 10-fold greater sampling size was used in this study; for the IFFLP model, the original 104 sampling produced 131 solutions, enough for the subsequent enrichment tests to be carried out. Results from additional sets of simulation and also from a run increasing the sample size to 10 fold, which increased the number of kinetic solutions to roughly 10 fold, indicated that the parameter motifs reported here had been reliably deduced (see Discussion).
Following Ma et al. , we discarded those parameter sets that render the model to produce extremely small steady-state values, persistent oscillations, weakly damped oscillations, and exceedingly long transient dynamics. For each of the remaining parameter sets (46,715 for NFBLB and 6,073 for IFFLP), the sensitivity and precision scores (i.e. equation (8) and equation (9) respectively) were calculated. We said a particular parameter set was a kinetic solution to the model if its sensitivity score was greater than 1 and its precision score greater than 10, as these criteria have been used to define perfect adaptation . It can be shown from equation (8) and (9) that these thresholds were chosen to ensure a stimulus of at least 20% of the initial steady-state value, and the system can return back to this value within an error of 2%, in consistence with those used in experimental measurements (Khan et al.  and Alon et al. ). More stringent thresholds reduced the value range of the parameter motifs, but the resultant minor changes did not significantly affect the main findings (see Discussion). We used computer programs from Ma et al.  and Matlab software (version 22.214.171.1244, release R2008a)  available at http://www.mathworks.com, to implement a computational pipeline to simulate both the NFBLB model and the IFFLP model numerically. We validated our simulation pipeline by reproducing the numerical results of  and also the steady-state solution of a four-node transcriptional regulation cascade of .
In order to see if there exists an underlying pattern in the values of kinetic parameters for the NFBLB model to yield perfect adaptation dynamics, we obtained the kinetic solutions and plotted the distribution of parameter values for each kinetic parameter. To test whether the resulting distributions of parameter values were enriched in the sets of kinetic solutions among those 105 (NFBLB) parameter sets sampled, we adopted an enrichment test that has found many uses in genomics sciences [43, 44]. For a given kinetic parameter, let N be the total number of parameter values sampled (here, N = 105 for NFBLB model), and let y i be the number of those in N belonging to the i th value class in the logarithm scale (i = 1, 2, …, 5); furthermore, let M be the number of kinetic solutions (here, M = 74 for NFBLB model), and x i be the number of those in M belonging to the same i th value class. Parameter values belonging to the 1st value class are within the interval [10-3, 10-2], those belonging to the 2nd value class are within [10-2, 10-1], and so on and so forth, with the 5th value class containing parameter values within [101, 102]. The five value classes of kinetic parameters may correspond to varying strengths of enzymatic reactions that can be measured and classified experimentally. Doubling the number of value classes resulted in a similar, albeit finer, map of parameter motifs, but did not alter the conclusions reached (see Discussion).
where i = 1, 2, 3, 4 and 5, and
As in the enrichment test employed in genomics sciences [43, 44], we can then compute the p-value to measure the statistical significance of the likelihood for observing x i when the null distribution (equation (10)) is assumed to be the true count distribution. In this study, we used a p-value threshold of 10-3 to decide the statistical significance of the enrichment test.
Thus, for each Michaelis-Menten constant K, we carried out five independent enrichment tests, each for each value class, and for each catalytic rate constant k, we carried out two independent enrichment tests, one for the 3rd value class (i.e. [10-1, 100]) and the other for the 4th value class (i.e. [100, 101]), due to the smaller range of parameter values for k (see above). If an enrichment test was statistically significant (p-value < 10-3), a motif in the form of value class was assigned to the kinetic parameter tested. To sum up, the outcome of this analysis produced motifs of kinetic parameters, which tells us whether a particular kinetic parameter is biased towards any specific value class on the logarithm scale, or none at all.
Functional association test and parameter inter-dependence
For each kinetic parameter, values from all the kinetic parameter sets (46,715 for NFBLB and 6,073 for IFFLP) were partitioned into two groups. The first group, called the motif group, consists of parameter values belonging to the biased value class(es) as identified by the above mentioned enrichment test on kinetic solutions; and the second group, called the non-motif group, comprises those parameter values that are not in the motif group.
We then tested whether the motif group exhibited higher sensitivity or precision scores than the non-motif group by comparing the score medians of the two groups. Since the scores were not normally distributed, we used the Mann–Whitney U-Test  for the analysis. The test produced a z-score, and we said a particular kinetic parameter is positively associated with the sensitivity or precision parts of the adaptation dynamics if the corresponding z-score is greater than 3.29 (i.e. the upper boundary of the critical value of the 99.9% confidence intervals). In this study our focus was on finding parameters that can significantly improve the function, although some of the parameters may exhibit a large negative z-score indicative of a negative role in the function. A bipartite kinetic-functionality network can then be constructed to display the associations between the kinetic motifs and the functionalities identified.
Finally, we investigated the cooperation between every pair of kinetic parameters. Specifically, we took the kinetic parameters from those 74 kinetic solutions (131 for IFFLP) and performed Pearson correlation test between the values of a pair of kinetic parameters that appeared in the kinetic motifs identified. We said two parameters are correlated if the p-value of the correlation test is less than 0.05.
Detecting kinetic motifs
As described in the Methods, we found only 74 sets of parameters from 105 randomly sampled sets that could satisfy the criteria of perfect adaptation dynamics for the NFBLB model. Figure 2 shows the distributions of these 74 sets of parameter values. We can see that while some parameters, k FBB especially, were limited to be within a relatively small range of values, others, like k FCC and K AC , saw a distribution covering nearly the entire range of the values sampled. On the whole, catalytic rate constants k FBB and k BA were biased towards the 3rd and the 4th value class, respectively, while all five Michaelis-Menten constants were biased towards one or more of the first three value classes. Other catalytic rate constants, namely k AB , k AC and k FCC , did not show apparent biases towards any vale classes. These observations were quantified with statistical significance by the enrichment tests; the results, summarized in Table 1, are consistent with the distributions of parameter values shown in Figure 2.
Functional roles of kinetic motifs
For each of the seven kinetic parameters showing bias to at least one value class with statistical significance as determined in Table 1, we carried out Mann–Whitney U-test  to find out whether a motif (i.e. a preferred value class) of that parameter is involved in the sensitivity function of the adaptation dynamics, or, correspondingly, whether the median of the sensitivity scores for the motif group is significantly larger than that for the non-motif group (see Methods). The same analysis was then repeated for precision.
The results, summarized in Table 2, indicate that three kinetic parameters, K AC , K FBB and K FCC , were highly significant in improving sensitivity scores, and six kinetic parameters, k BA , k FBB , K AB , K AC , K BA and K FCC , were highly significant in improving precision scores. Furthermore, for the majority of parameters, their motifs were either associated with improving sensitivity or precision scores, but not both. Two interesting exceptions are K AC and K FCC as their motifs tended to reflect improvements in both functionalities (Table 2). These observations are generally in accord with the results from an analytical analysis of the rate equations (see below and supplemental data). Note that sensitivity and precision are two conflicting dynamic processes with the former requiring the system to deviate from steady state abruptly and the latter requiring the system to return to the original steady state in a timely fashion (Figure 1A). Therefore, theoretically speaking, a parameter that improves one function will also have a negative effect on the other function, as reflected generally by the opposite signs of the z-scores obtained from the sensitivity and precision tests (Table 2). Finally, the above findings can be succinctly captured by drawing a kinetic-functionality network (Figure 3), which highlights both the functional roles and constraints (i.e. the enriched value classes) of kinetic parameters.
Cooperation of kinetic parameters
Next, we asked the question of whether kinetic parameters work independently or in a cooperative way with each other when contributing to the system’s adaptation dynamics. Figure 4 shows the results of correlation tests performed on all pairs of the seven kinetic parameters that exhibited value class biases. We identified one significant positive correlation (p-value < 0.05) between parameters k FBB and K BA , and four significant negative correlations in (k FBB , K AB ), (k FBB , K FCC ), (K AB , K FBB ) and (K BA , K FCC ) pairs. Interestingly, with the exception of K FBB , most of these correlated parameters contributed significantly to system’s precision (Figure 3), suggesting that they work in a cooperative manner in the precision mechanism of adaptation dynamics. In contrast, kinetic parameters contributing to the system’s sensitivity (i.e. K AC , K FBB and K FCC , see Figure 3) were not correlated with each other, implying that they function independently in the sensitivity mechanism. If the mathematical model employed can indeed simulate the mechanics of adaptation in real biological systems, a corollary of these findings is that precision seems to be a more complicated mechanism than sensitivity in the system, thus the former requires many parameters to work together in order to achieve the desired level of high precision.
Experimental data for kinetic parameters of E. coli chemotaxis
The NFBLB model is equivalent to the E. coli chemotaxis model with nodes A, B and C corresponding to the CheA-bound receptor complex, CheB and CheY, respectively. Chemotaxis of E. coli has been studied experimentally and parameters relating to individual processes involved in the model have been estimated [36–38, 46]. Intriguingly, as described below, the kinetic motifs observed here for the NFBLB model compared well with the experimental data for the E. coli chemotaxis (Table 3).
To facilitate and simplify the comparison, we dictated that parameters with a value in the first three value classes (i.e., < 100) are small-value parameters, while those in the 4th and 5th value class (i.e. ≧100) are large-value parameters. Note that in enzyme kinetics, an enzyme with a large K value (Michaelis-Menten constant) indicates a weak binding affinity to its substrate, while a large k value (catalytic rate constant) implies the occurrence of a rapid catalytic event . For sensitivity, the empirical estimates for K AC and K FCC , after being normalized with the concentration of CheY, were 0.36 and 0.006 respectively (Table 3). This echoes our finding that both parameters should take small values. K AC and K FCC are respectively involved in the rates of phosphorylation (i.e. activation) and dephosphorylation (i.e. deactivation) of the response regulator CheY. Goldbeter and Koshland  explored a simple model of enzyme reaction and found that if the activating and deactivating enzymes operate at saturation where the substrate concentration does not affect reaction rate, then an ultra-sensitivity response is observed. Similar arguments may apply to chemotaxis in E. coli: namely, in order to produce sensitivity dynamics, both phosphorylating and dephosphorylating agents (i.e. CheA and CheZ, respectively) must be saturated, implying a situation where the concentration of the substrate (i.e. CheY) cannot alter the reaction rate. A close inspection of the rate reaction for node C in equation (7) suggests that both K AC and K FCC taking on small values can fulfil this condition. Note that if both K AC and K FCC are small, then C> > K FCC and (1-C)> > K AC such that
and the concentration of node C (i.e. CheY) disappears from the rate equation completely.
The kinetic parameter K FBB is involved in the deactivation of node B in the NFBLB model and K FBB is also found to be biased to small values (1st value class motif in Table 1) for the model to exhibit sensitivity dynamics. Although node B of the NBFLP model corresponds to CheB in the chemotaxis of E. coli, to the best of our knowledge there are no natural enzymes reported to deactivate CheBp in the manner suggested by the NFBLB model. Perhaps an unrevealed enzyme exists to dephosphorylate CheBp, the phosphorylate form of CheB, or there might be other mechanism of CheBp dephosphorylation that is more complicated than the current knowledge can offer.
As for precision, the empirical estimates for K AB (normalized with the concentration of CheB), k FBB , K BA (normalized with the concentration of receptor complex) and k BA are 0.281, 0.35, 0.08 and 1.2, respectively (Table 3). These are also in agreement with our findings (Table 1) that K AB , k FBB and K BA are biased towards small values, and k BA is constrained to large values. K AB and k FBB are involved in the phosphorylation and dephosphorylation of CheB, respectively. According to Ma et al. , K AB is constrained to small values by the topological features of the NFBLB model such that the rate equation of node B (i.e. CheB) is independent of the input level I; this then implies the system is in a stable state independent of the initial perturbation and thus is able to maintain high precision level. From equation (7), a small value for k FBB can reduce the dephosphorylation rate of CheB, this in turn increases the deactivation rate of the receptor complex, thereby ensuing high precision. Finally, K BA and k BA play a part in the demethylation of the receptor complex, and intuitively the rate of its demethylation must be great (e.g. with a large k BA and a small K BA ) such that the perturbation initiated by the input signal can be mitigated in order to maintain high precision.
These observations of key parameters of the NFBLB model are furthermore supported by a number of experimental findings on the chemotaxis system of E. coli: 1) K FCC having a large effect on the sensitivity part of the system dynamics is in agreement with CheZ playing an important role in adjusting the concentration of CheY ; 2) K AC being an important kinetic parameter in affecting sensitivity agrees well with the receptor complex being a major contributor to sensitivity ; 3) CheB mutants being far less sensitive than the wild type due to the functional abnormality of the receptor complex in those mutants  implies that K FBB is an important parameter affecting sensitivity; 4) that phosphorylated CheB can increase the rate of receptor demethylation and thus speeds up adaptation  supports the finding that k BA , k FBB , K AB and K BA were all important parameters in contributing to the system’s precision mechanism.
We have developed here a methodology using parameter profiling and enrichment statistical tests to uncover not only the sets of kinetic parameters with which a model produces user-specified system dynamics, but also motifs (i.e. enriched value classes) of these parameters and their associations with specific functional aspects of the system’s dynamics. For these tasks, conventional methods usually focus on identifying the “best” parameter set in fitting the empirical data and on using complicated analytical explorations of models (e.g., sensitivity analysis) [52–54] or by a laborious local approach examining how changing the parameters one at a time would affect systems dynamics [55–57]. Note that the sensitivity analysis of conventional methods (not to confuse with the sensitivity of adaptation (Equation 8) studied in this work) is usually carried out for one specific output dynamics, whereas our profiling approach investigated the sensitivity of functional elements (sensitivity and precision of adaptation) for a collection of outpout dynamics (those that qualified as a perfect adaptation; there were 74 for the NFBLB model). Interestingly, the kinetic parameters showing value class biases (Table 2) are those exhibiting non-negligible sensitivity indices obtained from analytical derivation (Additional file 1: Equation S2) or from the numerical method implemented in AMIGO  (Additional file 1: Figure S1), the latter two being computed using the output dynamics and the parameter set of a randomly chosen one of the 74 kinetic solutions. Note that bootstrap-derived distributions of the kinetic parameters and their confidence intervals for this particular kinetic solution were generally in accord with the kinetic motifs deduced from the 74 kinetic solutions (Additional file 1: Figure S2). In summary, by profiling the parameters as a whole our method takes a global view to find not just one but clusters of viable parameter sets, thus moving a step further to account for the complexity of biological systems. Although a number of global-view approaches have recently been developed to sample from large and high dimensional parameter spaces, including a combined global and local exploration  and an approach with model checking on partitioned regions of parameters , these studies do not make inferences on whether motifs of parameters exist and how they might contribute to specific elements of the system dynamics. Our approach therefore offers a simple framework to systematically characterize and elucidate the functional contribution of kinetic parameters in a biological network.
The kinetic motifs obtained are quite robust in that only minor differences in their resolution were resulted from independent sampling runs (Additional file 1: Figure S3), different thresholds of the adaptation objectives (Additional file 1: Figure S4), and added number of value classes (Additional file 1: Figure S5). Further analysis showed that, for NFBLB and to satisfy the statistical significance of p-value < 10-3, 8 × 104 (rather than 105) sampling runs were required to converge and stabilize the kinetic motifs (Additional file 1: Figure S6). The computational cost of our method is dominated by the sampling and simulation step (see an analysis Additional file 1: Section III). To investigate the difficulties that will inevitably arise from larger networks for our method, we artificially linked two modules of NFBLB together (see Additional file 1: section IV) while requiring the system to produce the same adaptation dynamics as before. The results showed that 5 times of sampling/simulations (4 × 105 vs. 8 × 104) were needed to produce stabilized kinetic motifs (Additional file 1: Figure S7) for the twice-sized network (20 kinetic parameters vs. 10). However, it should be noted that the required number of sampling/simulations depends on many factors, including the specified output dynamics, the level of statistical significance desired, and the network topology (e.g., the IFFLP model needed 10 times less number of sampling/simulations than the NFBLB model to exhibit stabilized kinetic motifs, despite they both having 10 kinetic parameters). Note that our approach is quite general and can be integrated with other approaches. For instance, the Latin hypercube sampling (LHS) used here (and as in ) can be replaced by other methods, such as those mentioned above, to identify the kinetic solutions needed in the subsequent enrichment tests. Results from an experiment of combining LHS and genetic algorithm (GA) showed that 103 of LHS sampling followed by 100 generations of GA optimization yielded a similar set of kinetic motifs for NFBLB (Additional file 1: Table S1), suggesting that optimization can help to find more solutions from a smaller initial parameter set, but in this case the hybrid approach did not reduce the computational cost (since it also needed a total of 105 model evaluations), and could miss some of the marginally significant motifs (Additional file 1: Table S1). While further research is required to fully address the dimensionality problem of scaling up the system, complex biological networks are known to be composed of simple recurrent structural components [59–61]; a deeper understanding of these network components is an important first step toward a better understanding of the assemblage and functioning of a much larger system.
One interesting observation from the case studies of the NFBLB and the IFFLP (presented in Additional file 1: section VI) adaptation model is that the majority of parameters seem to contribute to only one single functionality (i.e. either sensitivity or precision, see Figure 3, Additional file 1: Figure S10). If the mathematical models are indeed mechanistic, this could have important biological implications as follows. The behavior or dynamics of a biological system is likely to be the result of intricate interactions of many biological processes. If a biological process has a major influence on all aspects of the systems behavior, then any changes to such a process may have a drastic impact on the system. Modularity is ubiquitous in biological systems as it provides an effective mechanism to corral damaging perturbations to local consequences . Thus, to ensure system robustness, evolution might have favored a biological system with a fine division of labors (i.e. modularity) among different biological components or processes [63–65]. Here, in the kinetic-functionality association, we may have uncovered yet another example of nature’s modularity design manifestated in the organization of kinetic parameters.
Previous studies have shown that certain types and arrangements of network structures are required to produce certain types of system dynamics [33, 66–68]; here, we have shown that, for a given network structure, certain types of values, or motifs, also exist for kinetic parameters in order to achieve specific system dynamics. Our results suggest that, as has been noted by others [69, 70], system dynamics can put constraints on the values of kinetic parameters. The discovery of these motifs underscores the intricate inter-relationships between structure (i.e. topology) of the biological network, kinetic parameters of the reactions involved, and the function of the biological system. Delineation of these relationships by methods such as the one developed here, which is general and can be applied to other types of well defined dynamics, will greatly advance our understanding of the design principles of prototype biological systems.
An increasing number of studies have revealed that complicated biological systems often share simple and universal design principles that are more understandable to biologists. The identification of motifs in biological networks is a prime example relating recurrent network structures to biological functions. Many studies have also argued for the importance of kinetic parameters in determining the dynamics of biological networks, but dissecting the association between system dynamics and kinetic parameters has been difficult. In this study, we have developed a methodology, akin to the enrichment analysis of gene expression profiles, to determine whether a preference of kinetic parameters adopting certain parameter values exists. Such preferences, or kinetic motifs, encapsulate the possible roles and functional constraints of kinetic parameters. Our analysis on models for the adaptation dynamics of the chemotaxis of Escherichia coli showed that design principles also exist from the perspective of kinetic parameters. Our methodology, owning to its generality and simplicity, provides a computational framework for understanding the kinetic mechanics of prototype biological networks.
Ideker T, Galitski T, Hood L: A new approach to decoding life: systems biology. Annu Rev Genomics Hum Genet. 2001, 2: 343-372. 10.1146/annurev.genom.2.1.343.
Kitano H: Systems biology: a brief overview. Science. 2002, 295 (5560): 1662-1664. 10.1126/science.1069492.
Weinberger LS, Burnett JC, Toettcher JE, Arkin AP, Schaffer DV: Stochastic gene expression in a lentiviral positive-feedback loop: HIV-1 Tat fluctuations drive phenotypic diversity. Cell. 2005, 122 (2): 169-182. 10.1016/j.cell.2005.06.006.
Sotiriou C, Piccart MJ: Opinion - Taking gene-expression profiling to the clinic: when will molecular signatures become relevant to patient care?. Nat Rev Cancer. 2007, 7 (7): 545-553. 10.1038/nrc2173.
Acar M, Mettetal JT, van Oudenaarden A: Stochastic switching as a survival strategy in fluctuating environments. Nat Genet. 2008, 40 (4): 471-475. 10.1038/ng.110.
Luo J, Emanuele MJ, Li D, Creighton CJ, Schlabach MR, Westbrook TF, Wong KK, Elledge SJ: A genome-wide RNAi screen identifies multiple synthetic lethal interactions with the Ras oncogene. Cell. 2009, 137 (5): 835-848. 10.1016/j.cell.2009.05.006.
Costanzo M, Baryshnikova A, Bellay J, Kim Y, Spear ED, Sevier CS, Ding H, Koh JL, Toufighi K, Mostafavi S: The genetic landscape of a cell. Science. 2010, 327 (5964): 425-431. 10.1126/science.1180823.
Spencer SL, Sorger PK: Measuring and modeling apoptosis in single cells. Cell. 2011, 144 (6): 926-939. 10.1016/j.cell.2011.03.002.
Chen KC, Calzone L, Csikasz-Nagy A, Cross FR, Novak B, Tyson JJ: Integrative analysis of cell cycle control in budding yeast. Mol Biol Cell. 2004, 15 (8): 3841-3862. 10.1091/mbc.E03-11-0794.
Palsson B: Systems biology: properties of reconstructed networks. 2006, Cambridge; New York: Cambridge University Press
Alon U: An introduction to systems biology: design principles of biological circuits. 2007, Chapman & Hall/CRC: Boca Raton, FL
Chuang HY, Hofree M, Ideker T: A decade of systems biology. Annu Rev Cell Dev Biol. 2010, 26: 721-744. 10.1146/annurev-cellbio-100109-104122.
Arkin AP, Schaffer DV: Network news: innovations in 21st century systems biology. Cell. 2011, 144 (6): 844-849. 10.1016/j.cell.2011.03.008.
Palsson B: Systems biology: simulation of dynamic network states. 2011, Cambridge, UK; New York: Cambridge University Press
Zamora-Sillero E, Hafner M, Ibig A, Stelling J, Wagner A: Efficient characterization of high-dimensional parameter spaces for systems biology. BMC Syst Biol. 2011, 5: 142-10.1186/1752-0509-5-142.
Chen BS, Chen PW: GA-based Design Algorithms for the Robust Synthetic Genetic Oscillators with Prescribed Amplitude, Period and Phase. Gene Regul Syst Biol. 2010, 4: 35-52.
Batt G, Yordanov B, Weiss R, Belta C: Robustness analysis and tuning of synthetic gene networks. Bioinformatics. 2007, 23 (18): 2415-2422. 10.1093/bioinformatics/btm362.
Berg HC, Brown DA: Chemotaxis in Escherichia coli analysed by three-dimensional tracking. Nature. 1972, 239 (5374): 500-504. 10.1038/239500a0.
Macnab RM, Koshland DE: The gradient-sensing mechanism in bacterial chemotaxis. Proc Natl Acad Sci USA. 1972, 69 (9): 2509-2512. 10.1073/pnas.69.9.2509.
Berg HC, Tedesco PM: Transient response to chemotactic stimuli in Escherichia coli. Proc Natl Acad Sci USA. 1975, 72 (8): 3235-3239. 10.1073/pnas.72.8.3235.
Mello BA, Tu Y: Perfect and near-perfect adaptation in a model of bacterial chemotaxis. Biophys J. 2003, 84 (5): 2943-2956. 10.1016/S0006-3495(03)70021-6.
Zigmond SH, Sullivan SJ: Sensory Adaptation of Leukocytes to Chemotactic Peptides. J Cell Biol. 1979, 82 (2): 517-527. 10.1083/jcb.82.2.517.
Shi W, Zusman DR: Sensory adaptation during negative chemotaxis in Myxococcus xanthus. J Bacteriol. 1994, 176 (5): 1517-1520.
Marwan W, Bibikov SI, Montrone M, Oesterhelt D: Mechanism of photosensory adaptation in Halobacterium salinarium. J Mol Biol. 1995, 246 (4): 493-499. 10.1006/jmbi.1994.0101.
Hilliard MA, Apicella AJ, Kerr R, Suzuki H, Bazzicalupo P, Schafer WR: In vivo imaging of C. elegans ASH neurons: cellular response and adaptation to chemical repellents. EMBO J. 2005, 24 (1): 63-72. 10.1038/sj.emboj.7600493.
Jaasma MJ, Jackson WM, Tang RY, Keaveny TM: Adaptation of cellular mechanical behavior to mechanical loading for osteoblastic cells. J Biomech. 2007, 40 (9): 1938-1945. 10.1016/j.jbiomech.2006.09.010.
Muzzey D, Gomez-Uribe CA, Mettetal JT, van Oudenaarden A: A systems-level analysis of perfect adaptation in yeast osmoregulation. Cell. 2009, 138 (1): 160-171. 10.1016/j.cell.2009.04.047.
Spehr J, Hagendorf S, Weiss J, Spehr M, Leinders-Zufall T, Zufall F: Ca2+ − calmodulin feedback mediates sensory adaptation and inhibits pheromone-sensitive ion channels in the vomeronasal organ. J Neurosci. 2009, 29 (7): 2125-2135. 10.1523/JNEUROSCI.5416-08.2009.
Barkai N, Leibler S: Robustness in simple biochemical networks. Nature. 1997, 387 (6636): 913-917. 10.1038/43199.
Yi TM, Huang Y, Simon MI, Doyle J: Robust perfect adaptation in bacterial chemotaxis through integral feedback control. Proc Natl Acad Sci USA. 2000, 97 (9): 4649-4653. 10.1073/pnas.97.9.4649.
Wadhams GH, Armitage JP: Making sense of it all: Bacterial chemotaxis. Nat Rev Mol Cell Biol. 2004, 5 (12): 1024-1037. 10.1038/nrm1524.
Porter SL, Wadhams GH, Armitage JP: Signal processing in complex chemotaxis pathways. Nat Rev Microbiol. 2011, 9 (3): 153-165. 10.1038/nrmicro2505.
Ma WZ, Trusina A, El-Samad H, Lim WA, Tang C: Defining Network Topologies that Can Achieve Biochemical Adaptation. Cell. 2009, 138 (4): 760-773. 10.1016/j.cell.2009.06.013.
Sourjik V, Berg HC: Binding of the Escherichia coli response regulator CheY to its target measured in vivo by fluorescence resonance energy transfer. Proc Natl Acad Sci USA. 2002, 99 (20): 12669-12674. 10.1073/pnas.192463199.
Iman RL, Helton JC, Campbell JE: An Approach to Sensitivity Analysis of Computer-Models.1. Introduction, Input Variable Selection and Preliminary Variable Assessment. J Qual Technol. 1981, 13 (3): 174-183.
Kollmann M, Lovdok L, Bartholome K, Timmer J, Sourjik V: Design principles of a bacterial signalling network. Nature. 2005, 438 (7067): 504-507. 10.1038/nature04228.
Morton-Firth CJ, Shimizu TS, Bray D: A free-energy-based stochastic simulation of the Tar receptor complex. J Mol Biol. 1999, 286 (4): 1059-1074. 10.1006/jmbi.1999.2535.
Rao CV, Kirby JR, Arkin AP: Design and diversity in bacterial chemotaxis: a comparative study in Escherichia coli and Bacillus subtilis. PLoS Biol. 2004, 2 (2): E49-10.1371/journal.pbio.0020049.
Khan S, Castellano F, Spudich JL, McCray JA, Goody RS, Reid GP, Trentham DR: Excitatory signaling in bacterial probed by caged chemoeffectors. Biophys J. 1993, 65 (6): 2368-2382. 10.1016/S0006-3495(93)81317-1.
Alon U, Surette MG, Barkai N, Leibler S: Robustness in bacterial chemotaxis. Nature. 1999, 397 (6715): 168-171. 10.1038/16483.
Henson R, Cetto L: The MATLAB bioinformatics toolbox. Encyclopedia of Genetics, Genomics, Proteomics and Bioinformatics. 2005, Natick, MA, USA: The MathWorks, Inc
Chiang AWT, Hwang MJ: A computational pipeline for identifying kinetic motifs to aid in the design and improvement of synthetic gene circuits. BMC Bioinformatics. 2013, 14 (Suppl 16): S5-10.1186/1471-2105-14-S16-S5.
Mootha VK, Lindgren CM, Eriksson KF, Subramanian A, Sihag S, Lehar J, Puigserver P, Carlsson E, Ridderstrale M, Laurila E: PGC-1alpha-responsive genes involved in oxidative phosphorylation are coordinately downregulated in human diabetes. Nat Genet. 2003, 34 (3): 267-273. 10.1038/ng1180.
Subramanian A, Tamayo P, Mootha VK, Mukherjee S, Ebert BL, Gillette MA, Paulovich A, Pomeroy SL, Golub TR, Lander ES: Gene set enrichment analysis: a knowledge-based approach for interpreting genome-wide expression profiles. Proc Natl Acad Sci USA. 2005, 102 (43): 15545-15550. 10.1073/pnas.0506580102.
Wilcoxon F: Individual Comparisons by Ranking Methods. Biometrics Bull. 1945, 1 (6): 80-83. 10.2307/3001968.
Vuppula RR, Tirumkudulu MS, Venkatesh KV: Mathematical modeling and experimental validation of chemotaxis under controlled gradients of methyl-aspartate in Escherichia coli. Mol Biosyst. 2010, 6 (6): 1082-1092. 10.1039/b924368b.
Stewart RC: Activating and inhibitory mutations in the regulatory domain of CheB, the methylesterase in bacterial chemotaxis. J Biol Chem. 1993, 268 (3): 1921-1930.
Stewart RC, Jahreis K, Parkinson JS: Rapid phosphotransfer to CheY from a CheA protein lacking the CheY-binding domain. Biochemistry. 2000, 39 (43): 13157-13165. 10.1021/bi001100k.
Rogers A, Gibon Y: Chapter 4. Enzyme kinetics: theory and practice. Plant metabolic networks. Edited by: Schwender J. 2009, New York: Springer, 71-103.
Goldbeter A, Koshland DE: An amplified sensitivity arising from covalent modification in biological systems. Proc Natl Acad Sci USA. 1981, 78 (11): 6840-6844. 10.1073/pnas.78.11.6840.
Lupas A, Stock J: Phosphorylation of an N-terminal regulatory domain activates the CheB methylesterase in bacterial chemotaxis. J Biol Chem. 1989, 264 (29): 17337-17342.
Li ZF, Osborne MR, Prvan T: Parameter estimation of ordinary differential equations. Ima J Numer Anal. 2005, 25 (2): 264-285. 10.1093/imanum/drh016.
Chou IC, Voit EO: Recent developments in parameter estimation and structure identification of biochemical and genomic systems. Math Biosci. 2009, 219 (2): 57-83. 10.1016/j.mbs.2009.03.002.
Schellenberger J, Zielinski DC, Choi W, Madireddi S, Portnoy V, Scott DA, Reed JL, Osterman AL, Palsson B: Predicting outcomes of steady-state 13C isotope tracing experiments using Monte Carlo sampling. BMC Syst Biol. 2012, 6: 9-10.1186/1752-0509-6-9.
Gonze D, Halloy J, Goldbeter A: Robustness of circadian rhythms with respect to molecular noise. Proc Natl Acad Sci USA. 2002, 99 (2): 673-678. 10.1073/pnas.022628299.
Zak DE, Stelling J, Doyle FJ: Sensitivity analysis of oscillatory (bio)chemical systems. Comput Chem Eng. 2005, 29 (3): 663-673. 10.1016/j.compchemeng.2004.08.021.
Szallasi Z, Stelling J, Periwal V: System modeling in cell biology: from concepts to nuts and bolts. 2006, Cambridge, Mass: MIT Press
Balsa-Canto E, Banga JR: AMIGO, a toolbox for advanced model identification in systems biology using global optimization. Bioinformatics. 2011, 27 (16): 2311-2313. 10.1093/bioinformatics/btr370.
Wolf DM, Arkin AP: Motifs, modules and games in bacteria. Curr Opin Microbiol. 2003, 6 (2): 125-134. 10.1016/S1369-5274(03)00033-X.
Alon U: Network motifs: theory and experimental approaches. Nat Rev Genet. 2007, 8 (6): 450-461. 10.1038/nrg2102.
Tyson JJ, Novak B: Functional motifs in biochemical reaction networks. Annu Rev Phys Chem. 2010, 61: 219-240. 10.1146/annurev.physchem.012809.103457.
Kitano H: Biological robustness. Nat Rev Genet. 2004, 5 (11): 826-837. 10.1038/nrg1471.
Hartwell LH, Hopfield JJ, Leibler S, Murray AW: From molecular to modular cell biology. Nature. 1999, 402 (6761 Suppl): C47-C52.
Ihmels J, Friedlander G, Bergmann S, Sarig O, Ziv Y, Barkai N: Revealing modular organization in the yeast transcriptional network. Nat Genet. 2002, 31 (4): 370-377.
Schlosser G, Wagner GP: Modularity in development and evolution. 2004, Chicago: University of Chicago Press
Shen-Orr SS, Milo R, Mangan S, Alon U: Network motifs in the transcriptional regulation network of Escherichia coli. Nat Genet. 2002, 31 (1): 64-68. 10.1038/ng881.
Brandman O, Meyer T: Feedback loops shape cellular signals in space and time. Science. 2008, 322 (5900): 390-395. 10.1126/science.1160617.
Tsai TY, Choi YS, Ma W, Pomerening JR, Tang C, Ferrell JE: Robust, tunable biological oscillations from interlinked positive and negative feedback loops. Science. 2008, 321 (5885): 126-129. 10.1126/science.1156951.
Famili I, Forster J, Nielsen J, Palsson BO: Saccharomyces cerevisiae phenotypes can be predicted by using constraint-based analysis of a genome-scale reconstructed metabolic network. Proc Natl Acad Sci USA. 2003, 100 (23): 13134-13139. 10.1073/pnas.2235812100.
Liu J: Kinetic constraints for formation of steady states in biochemical networks. Biophys J. 2005, 88 (5): 3212-3223. 10.1529/biophysj.104.056085.
We thank Dr. Chao Tang of the Department of Bioengineering and Therapeutic Sciences, UCSF, and Dr. Wenzhe Ma of the Department of Systems Biology, Harvard Medical School, for making their computer programs available to us. AWTC is grateful to Prof. Bernhard Ø. Palsson of the Department of Bioengineering, UCSD, and members of his lab, Mr. Aarash Bordbar in particular, for helpful discussions and assistance in this study during his visit.
The authors declare that they have no competing interests.
Conceived and designed the experiments: AWTC MJH. Performed the experiments: AWTC. Analyzed the data: AWTC WCL PC MJH. Wrote the paper: AWTC WCL PC MJH. This work was supported by the Taiwan International Graduate Program and a grant from the National Science Council of Taiwan (NSC grant no. 100-2311-B-001-021) to MJH, and also by a visiting student fellowship to AWTC (NSC grant no. NSC98-2917-I-010-102). All authors read and approved the final manuscript.
Electronic supplementary material
Additional file 1:(I) Mechanisms of functional associations for the NFBLB model; (II) Additional analysis for the NFBLB model. Figure S1-S6; (III) An analysis of computational cost; (IV) Simulation for a model of two linked NFBLPs (NFBLP2). Figure S7; (V) Results for GA-augmented simulations of the NFBLP model. Table S1; (VI) Results for the IFFLP model. Figure S8-S11 and Table S2-S3. (PDF 2 MB)
About this article
Cite this article
Chiang, A.W., Liu, W., Charusanti, P. et al. Understanding system dynamics of an adaptive enzyme network from globally profiled kinetic parameters. BMC Syst Biol 8, 4 (2014). https://doi.org/10.1186/1752-0509-8-4
- Kinetic motif
- Parameter profile
- Biological network
- Systems biology