Nucleic acid-based constitutional dynamic networks (CDNs) have recently emerged as versatile tools to control a variety of catalytic processes. A key challenge in the application of these systems is achieving intercommunication between different CDNs to mimic the complex interlinked networks found in cellular biology. In particular, the possibility to interface photochemical ‘energy-harvesting’ processes with dark-operating ‘metabolic’ processes, in a similar way to plants, represents an up to now unexplored yet enticing research direction. The present study introduces two CDNs that allow the intercommunication of photocatalytic and dark-operating catalytic functions mediated by environmental components that facilitate the dynamic coupling of the networks. The dynamic feedback-driven intercommunication of the networks is accomplished via information transfer between the two CDNs effected by hairpin fuel strands in the environment of the system, leading to the coupling of the photochemical and dark-operating modules.
The regulation of complex processes by dynamic networks is a defining feature of cellular biology1,2,3,4,5. The ability of these biomolecular networks to reconfigure in response to environmental triggers provides a mechanism for the stimuli-driven control of many cellular functions, such as the spatiotemporal regulation of gene expression6,7,8,9,10. There is great interest in mimicking such networks using artificial means (systems chemistry) in order to emulate natural processes towards the development of synthetic biomimetic systems11,12,13,14,15. In particular, complex networks of interconnected systems synchronized with the environment play important roles in the enhanced fitness and growth vigor of plants, and understanding the dynamic molecular mechanisms regulating plant metabolism, photosynthesis and growth is a continuous scientific challenge16,17. Substantial research efforts are directed towards the development of constitutional dynamic networks (CDNs) emulating functions of native network assemblies12,18,19,20. The simplest [2×2] CDN consists of four dynamically interchangeable and equilibrated constituents AA′, AB′, BA′, and BB′. The triggered stabilization of one of the constituents, e.g., AA′ results in the adaptive dynamic reconfiguration of the CDN into a new equilibrated network, where the content of AA′ is enriched at the expense of AB′ and BA′, which each share components with AA′. The dynamic separation of AB′ and BA′ leads to the recombination of B and B′ and the enrichment of BB′. Different molecular and macromolecular CDNs revealing adaptive reconfiguration features triggered by light21,22, temperature23, electrical field24, pH23, and supramolecular H-bonds25 were reported, and constitutional dynamic libraries and dynamic reaction networks26,27,28,29,30 were demonstrated. Recently, we have introduced DNA-based CDNs as a versatile approach for the regulation of a variety of catalytic processes and functional materials31. DNA structures are well-suited towards the design of CDNs, as the base sequence comprising the nucleic acid strands provides a rich toolbox to control the stabilization, destabilization, and reconfiguration of the CDN constituents, for example by fuel/anti-fuel strands32, the K+-ion/crown ether mediated formation/dissociation of G-quadruplexes33, and the reversible stabilization/destabilization of duplexes by photoisomerizable intercalator units34. By engineering the constituents of DNA-based CDNs to perform specific functions, control over their activity may be achieved through the dynamic changes of the composition of the CDN in response to specific triggers. For example, the guided transcription of mRNA and the translation of proteins by a [2×2] CDN was recently achieved35. Many biological networks, however, do not operate in isolation but function as part of larger ensembles in which the triggered reconfiguration of one network proceeds with concomitant information transfer to influence the activity of associated networks. By extension, a second network may subsequently regulate the composition of the first, thus enabling a feedback mechanism. Indeed, we have recently demonstrated the feedback-driven regulation of orthogonal enzymatic cascades through the guided intercommunication of two stimuli-responsive CDNs36. Beyond the coupling of enzymatic reactions, however, the challenge remains to develop the CDN systems to mimic further biological processes of enhanced complexity. The photosynthetic network in plants is tightly coupled to photorespiration and assimilation networks37, and to the overall plant metabolic machinery38,39 and the inter-relationships between the photosynthetic apparatus and the coupled dark networks reveal complex intercommunication patterns40. Until now, however, the challenge of achieving the CDN-regulated intercommunication between a photochemical function and a dark-operating function reminiscent of this natural machinery has not yet been addressed. We envisaged that DNA-based CDNs could serve as a means to interlink energy-harvesting and metabolic processes as a step towards emulating the native machinery found in plants.
In the present study, we introduce CDNs as functional modules to control the integration of photochemical and dark-operating processes, mediated through auxiliary fuel strands in the environment of the CDNs. A CDN-guided “photosynthetic” network that drives the light-induced electron transfer (ET) and the photosynthesis of NADPH is coupled to a dark-operating ‘metabolic’ CDN assembly that stimulates the biocatalytic oxidation of lactate to pyruvate and the cascaded metabolic amination of pyruvate to l-alanine. We demonstrate the intercommunication between the photochemical and dark-operating networks afforded by the environmental components, where the CDN that drives the enhanced photosynthesis of NADPH also interacts with an auxiliary strand to generate the signal that reconfigures the second network accelerating the metabolic process. This CDN-driven enhancement of the metabolic network, in turn, leads to a positive feedback signal to the first network that dictates the complementary acceleration of the photosynthetic process. Thus, interlinking the two networks via the environmental fuel strands provides a means for the dynamic coupling of two distinct biomimetic transformations that emulate the photosynthetic and dark-operating machinery of plant cells.
A photosynthetic CDN
Fig. 1a introduces the dynamic photocatalytic module mimicking photosynthesis, CDN X. The network consists of four constituents where the photosensitizer Zn(II)-protoporphyrin IX (Zn-PPIX) intercalates into the G-quadruplex unit, tethered as photosensitizer to component A of constituent AA′, and the N,N’-dialkyl-4,4’-bipyridinium (V2+) electron acceptor is covalently linked to component A′ of constituent AA′ (Supplementary Figs. 1–2). Irradiation of the photocatalytic module results in the effective quenching of the photosensitizer to yield the redox intermediates Zn-PPIX+·/GQ and V+· (Fig. 1a, panel I). In the presence of 1,4-nicotinamide adenine dinucleotide phosphate (NADP+) and ferredoxin-NADP+-reductase (FNR), the formation of reduced cofactor NADPH proceeds, in analogy to the photosystem I. Each of the constituents in CDN includes a loop domain, used to shift the CDN equilibrium through the stabilization of a triplex upon addition of the appropriate trigger strand, panel II. In addition, each of the constituents is engineered to include a different Mg2+-dependent DNAzyme reporter unit to cleave fluorophore-quencher ribonucleobase-modified substrates for the quantitative evaluation of the concentrations of constituents, panel III.
Fig. 1a and Supplementary Fig. 3 depict the triggered reconfiguration of CDN X in the presence of auxiliary triggers. Subjecting CDN X to the strand T1 leads to the stabilization of the T-A.T triplex structure in the loop domain, resulting in the stabilization of AA′ and the reconfiguration of CDN X into CDN Xa, where AA′ is upregulated, constituents AB′ and BA′ are downregulated and the constituent BB′ is upregulated (Supplementary Figs. 4–6). The reverse displacement of the trigger T1 by the counter trigger T1′ regenerates CDN X. Similarly, treatment of CDN X with the trigger T2 stabilizes the constituent BA′. BA′ and AB′ are upregulated, and AA′ and BB′ are downregulated (Supplementary Fig. 6). The treatment of CDN Xb with the counter trigger T2′ restores CDN X. The quantitative contents of the constituents in different CDNs are shown in Fig. 1b and Supplementary Table 1. The photosensitized ET process proceeding in different CDNs is stimulated by constituent AA′. The absorption spectra of the photogenerated V+· (Fig. 1c) reveal that the T1-upregulated constituent AA′ in CDN Xa leads to the enhanced photoinduced ET, whereas the T2-downregulation of AA′ in CDN Xb reduces the photoinduced ET. Fig. 1d demonstrates the switchable and reversible control over the photoinduced ET process guided by the T1-/T2-triggered reconfiguration of the CDN modules. The secondary CDN-guided synthesis of NADPH driven by the primary photoinduced V+·, in the presence of FNR, NADP+, and mercaptoethanol (electron donor), is presented in Fig. 1e–g. The time-dependent build-up of NADPH (λ = 345 nm) and V+· (λ = 395 nm) is observed. It is evident that the build-up of NADPH by CDN Xa (Fig. 1f) is enhanced as compared with the NADPH generated by CDN X (Fig. 1e), whereas the build-up of NADPH by CDN Xb (Fig. 1g) is reduced as compared to CDN X. Fig. 1h shows the time-dependent formation of NADPH at time intervals of illumination of CDNs X, Xa, and Xb. The efficiency of production of the photogenerated NADPH is controlled by the efficiency of the primary photoinduced ET process that yields V+·.
A metabolic CDN
The metabolic CDN module is introduced in Fig. 2 and Supplementary Fig. 7. CDN Y is composed of the constituents CC′, DC′, CD′ and DD′, where the components of DD′ are modified with lactate dehydrogenase (LDH) and NAD+, Supplementary Figs. 2, 8. The metabolic biocatalytic transformation proceeding in CDN Y involves the LDH-biocatalyzed reduction of NAD+ to NADH by lactic acid, and the concomitant formation of pyruvic acid. The biocatalyzed formation of NADH is coupled to the secondary reduction of methylene blue (MB+) to colorless MBH, a process that allows the spectroscopy readout of the time-dependent formation of NADH (Fig. 2a, panel I). In addition, the biocatalyzed formation of NADH and pyruvic acid is coupled to the secondary reductive amination of pyruvic acid, in the presence of NH4+ and alanine dehydrogenase (AlaDH), to form l-alanine as a metabolic product.
Subjecting CDN Y to trigger T3 stabilizes constituent DD′, resulting in the reconfiguration of CDN Y to CDN Ya, where DD′ is upregulated, DC′ and CD′ are downregulated and CC′ is upregulated (Supplementary Figs. 9–11). The reverse treatment of CDN Ya with T3′ displaces T3 from DD′ and results in the regeneration of CDN Y. In addition, treatment of CDN Y with T4 stabilizes the constituent CD′, leading to the reconfiguration of CDN Y to CDN Yb, where CD′ and DC′ are upregulated and the constituents CC′ and DD′ are downregulated. Fig. 2b and Supplementary Table 2 show the concentrations of the constituents. The CDNs-guided time-dependent operation of the biocatalytic cascade corresponding to LDH-catalyzed reduction of NAD+ by lactic acid to NADH, and the subsequent reduction of MB+ (λ = 630 nm) are presented in Fig. 2c and Supplementary Figs. 12–13. The time-dependent reduction of MB+ to MBH is enhanced, in the presence of the T3-triggered reconfigured CDN Ya, and depleted in the presence of the T4-reconfigured CDN Yb, consistent with the upregulation of the constituent DD′ in CDN Ya and the downregulation of DD′ in CDN Yb, respectively. In addition, Fig. 2d presents the time-dependent CDNs-driven metabolic cascade, where the LDH-biocatalyzed reduction of NAD+ to NADH by lactate is followed by the AlaDH-catalyzed amination of the generated pyruvic acid to yield l-alanine (Supplementary Figs. 14–15, Supplementary Tables 3–5). The rate of formation of l-alanine metabolite is enhanced in the presence of CDN Ya and dampened by CDN Yb, respectively.
Intercommunicated photosynthetic and metabolic dynamic networks
In the next step, efforts to couple the photosynthetic module and the dark-operating metabolic module were undertaken. The principle to intercommunicate the two modules is displayed in Fig. 3a. The constituents BB′ and CC′ in CDNs X and Y were each pre-engineered to include extra Mg2+-dependent DNAzyme units. These units are termed activators, integrated into the composite in order to intercommunicate the networks. To intercommunicate the networks, we added two hairpins, Ha or Hd into the mixture of two CDNs. The Ha is designed to be cleaved by the activator in constituent CC′ to yield the fragmented strand Ha-1 that interacts with constituent AA′ by the stabilization of the triplex T-A·T in the loop domain of AA′ (Fig. 3a route I and Supplementary Fig. 16). This results in the upregulation of AA′ and BB′ and downregulation of AB′ and BA′ (Supplementary Figs. 17–18). That is, the cleavage of Ha by the metabolic module is anticipated to enhance the performance of the photosynthetic module by upregulating AA′. On the other hand, the cleavage of hairpin Hd by the activator of constituent BB′ yields the fragmented strand Hd-1 that provides an information strand to control the activity of CDN Y (Fig. 3a route II and Supplementary Fig. 19). The binding of Hd-1 to the loop domain of DD′, and the formation of the T-A·T triplex lead to the stabilization of DD′, the upregulation of DD′ and CC′ and the downregulation of CD′ and DC′ (Supplementary Figs. 20–21). The resulting time-dependent upregulation of DD′ leads, then, to a time-dependent increase in the metabolic performance of CDN Y.
In the first step, the unidirectional intercommunication between the networks using hairpin Ha or Hd was evaluated. Fig. 3b and Supplementary Figs. 22–23 show the formation of NADPH by the photosynthetic module upon exposure to Ha-1 generated by CDN Y at different time intervals. As the time interval is prolonged, the photosensitized generation of NADPH by the photosynthetic CDN X/FNR is enhanced, consistent with the continuous enrichment of the constituent AA′ by Ha-1. Fig. 3c depicts the metabolic performance of CDN Y before and after the strand Ha-1 was supplied to CDN X, by following the reduction of MB+ to MBH. As expected, the metabolic module is unaffected upon supplying Ha-1 as a trigger to CDN X. Fig. 3d shows the rate of synthesis of l-alanine by CDN Y upon feeding the two CDNs with Hd-1 generated at different time intervals (Supplementary Figs. 24–25, Supplementary Tables 6–9). As the time interval of the generation of Hd-1 is prolonged, the synthesis of l-alanine is enhanced, consistent with the stabilization and time-dependent overexpression of DD′, in the presence of Hd-1. Fig. 3e shows the spectra of NADPH generated by the photosynthetic module (1-h irradiation) before and after the generation of Hd-1, implying CDN X is unaffected upon the transfer of the information strand (Hd-1) to CDN Y. Note that this discussion introduces the positive intercommunication dialog between the CDNs. One may envisage, however, the negative intercommunication between the CDNs. For example, subjecting coupled CDNs to hairpin Hn (cleaved by the activator of BB′) leads to the generation of fragmented product Hn-1 that stabilizes CD′, the downregulation of DD′ proceeds, resulting in the inhibition of the metabolic module (Supplementary Figs. 26–29). It should be noted that probing the effect of Ha on the metabolic module by means of the methylene blue probe is examined in the dark, without activation of the photosynthetic network, and thus NADPH is not formed and the only source of the methylene blue reducing agent (NADH) originates from the dark LDH-catalyzed oxidation of lactate. Furthermore, upon running the metabolic cycle module composed of lactate/LDH/AlaDH, the equilibrated content of NADH is negligible and does not affect the spectrum of NADPH generated by the photosynthetic module.
Next, we subjected the mixture of the two CDNs to the two hairpins simultaneously. This has a significant effect on the intercommunication between the two CDNs (Fig. 4a). The cleavage of the hairpin Ha yields the strand Ha-1 that provides the information to upregulate AA′ in the photosynthetic module, leading to the time-dependent increase in the photosensitized ET process and the FNR-catalyzed synthesis of NADPH. However, the upregulation of AA′ is also accompanied by the upregulation of BB′ that leads to the time-dependent enhancement of the cleavage of Hd to form Hd−1. The latter product provides the information strand to enhance the metabolic module synthesizing l-alanine. The stabilization and upregulation of DD′ are accompanied in turn by the upregulation of CC′ and, thus, increased cleavage of Ha and the enhancement of the photosynthetic module takes place. In the presence of the hairpins Ha and Hb, a positive feedback mechanism intercommunicating the CDNs is established (Supplementary Figs. 30–32 and Supplementary Note). Fig. 4b and Supplementary Figs. 33–34 show the photosensitized-NADPH generated at time intervals of the feedback-driven intercommunication of the two networks, indicating the generation of NADPH by the photosynthetic module is enhanced. Fig. 4c depicts the rates of the metabolic path (lactate/LDH/NAD+/MB+ cascade) at time intervals of the intercommunication between the networks. As the feedback process enriches AA′ and DD′, the concentration of NADPH is higher and the biocatalytic cascade is enhanced. The results demonstrate a tight relation between the photosynthetic module and the dark-operating module. The upregulation of the photoresponsive constituent of CDN X is accompanied by increased generation of the information transferring strand (via cleavage of Hd) that upregulates the metabolic constituent of CDN Y. This leads to a positive feedback mechanism since this reconfiguration of CDN Y, in turn, accelerates the cleavage of Ha, which acts as the informational trigger to further enhance the upregulation of the photosynthetic constituent of the first network. It should be noted that the hairpins Ha and Hd that intercommunicate the networks can not be regenerated and they act as fuel strands that control the compositions of the networks while generating degraded waste products.
It should be noted, however, that in contrast to natural photosynthesis, where light triggers the intercommunication of the photosynthetic and metabolic modules, the present study applies chemical fuel strands, generated by cleavage of the hairpin structures, as intercommunicating activators. Nonetheless, recent advances in operating dynamic networks demonstrated the light-induced separation of trans-azobenzene stabilized nucleic acid duplexes by photoisomerization of trans-units into the cis-azobenzene state34. Such photochemical transformation could mimic the natural system by providing photogenerated fuels that guide the intercommunication of the networks. In addition, the blockage of the photosynthetic module in nature (dark conditions), inhibits autonomously the carbon assimilation process, a feature missing in the present intercommunicated artificial networks, owing to the irreversible formation of the cleaved hairpin fuel strands. This limitation could be resolved, however, by applying photoisomerizable activator strands, such as the cis-azobenzene trigger. The intrinsic dark back isomerization of the cis-azobenzene strand to the trans-state could then provide an autonomous path to inhibit the metabolic cycle, in analogy to inhibition of the carbon assimilation process under dark conditions of the photosynthetic apparatus.
A further drawback of the present light/dark intercommunicating networks originates from the operation of the coupled CDNs under thermodynamic control. This leads to a permanent background output of the CDNs, and to a limited dynamic range of the switching performance of the coupled networks, far lower than in nature. A strategy to overcome this limitation could involve the activation of the photosynthetic/metabolic networks under out-of-equilibrium, dissipative conditions. Indeed, the operation of dissipative CDNs and of gated networks was recently reported41,42, providing a potential path to follow.
The study introduces two complementary dynamic networks that perform photocatalytic and dark-operating functions, thus adding an additional level of complexity compared to previously reported systems that allow only the control of enzymatic reactions36. One network introduces a photosynthetic path, where the control over the light-induced ET and the subsequent catalyzed synthesis of NADPH proceeds, in analogy to the transformation driven by photosystem I. A second dynamic network demonstrates a metabolic path by the input-driven oxidation of lactate and its metabolic transformation to l-alanine. The two networks are intercommunicated, demonstrating the guided activation of the metabolic network by an auxiliary component of the photosynthetic network and the counter control over the photosynthetic network by means of the metabolic network. Finally, the integrated feedback-driven operation of the photosynthetic network and the metabolic network is established by introducing the coupled operation of the two networks, where information transfer between them, mediated by fuel strands in the network environment, exists. Beyond highlighting the integration of the photochemical and dark-operating networks reminiscent of native biological transformations, the study introduces an important path to guide the synthesis of useful materials (l-alanine) by the metabolic network43. Beyond advancing System Chemistry by introducing artificial dynamic networks mimicking the photosynthetic/plant metabolic processes, important challenges are ahead of us. These include the photochemical coupling of the photosynthetic and metabolic modules and the development of gated and cascaded, dissipative, out-of-equilibrium photosynthetic/metabolic networks.
Modification of strand A′ with V2+
In all, 60 μL of 0.05 M V2+ (10 eq) and 30 μL of 0.01 M sulfo-EMCS (1 eq) were mixed in phosphate-buffered saline (20 mM, pH = 7.24) and incubated at room temperature for 1 h. Then 30 μL of 1 mM strand A′ (0.1 eq) was added and incubated for another 2 h. Excess reactants were removed using Amicon 10 kD cutoff filters. The synthesis route was shown in Supplementary Fig. 2a. The characterization of the modified strand is shown in Supplementary Figs. 35, 36, and Supplementary Table 10.
Modification of strand D with LDH
In all, 10 µM of LDH and 1.2 mM SPDP in HEPES buffer (10 mM, pH = 8) were incubated for 1 h. Excess SPDP was removed using Amicon 30 kD cutoff filters. Before modification of strand D with LDH, strand D was treated with TCEP (100-fold excess) for 2 h and washed by using Amicon 3 kD cutoff filters. Next, SPDP-modified LDH was conjugated to strand D (eightfold excess) through a disulfide bond exchange of the activated pyridyldithiol group (see synthetic scheme in Supplementary Fig. 2b). The reaction was performed in HEPES buffer (10 mM, pH = 8) for 2 h. The SPDP coupling efficiency was evaluated by monitoring the increase in absorbance at 343 nm owing to the release of pyridine-2-thione (Supplementary Fig. 10a, b, extinction coefficient: 8080 M−1 cm−1). Excess DNA was removed using Amicon 30 kD cutoff filters. The enzymatic activity of DNA-modified LDH was ~75% of the activity of the native enzyme (Supplementary Fig. 10c). The DNA labeling ratio of the purified enzyme-DNA conjugates was estimated by measuring the absorbance at 260 and 280 nm (Supplementary Fig. 37 and Supplementary Table 11) and mass analysis was shown in Supplementary Fig. 38.
Modification of strand D′ with NAD+
The preparation of D′-NAD+ (see synthetic scheme in Supplementary Fig. 2c) was in the following. In all, 4-carboxyphenylboronic acid (1.8 µL, 50 mM) reacted with EDC (2.3 µL, 10 mg/mL) in 200 µL of MES buffer (10 mM, pH = 5.5) for 5 min, subsequently NHS (3.5 µL, 10 mg/mL) was added and reacted for 10 min. Then, D′ (2.3 µL, 4.4 mM) and NAD+ (3 µL, 5 mM) were added, stirring for 2 h and kept at 4°C overnight. Excess reactants were washed away with Amicon 10 kD cutoff filters.
Preparation of CDNs
A sample of 1 mL of CDN (each component 2 µM) was taken as an example to explain the procedure of the preparation of CDNs:
CDN X, including the constituents AA′, BB′, AB′, BA′, was prepared as follows: A (20 µL, 100 µM), A′ (20 µL, 100 µM), B (20 µL, 100 µM), B′ (20 µL, 100 µM) and PPIX (2 µL, 1 mM) were mixed in Tris buffer (10 mM, pH = 7.29) that includes 20 mM MgCl2 and 100 mM K+. The mixture was annealed at 37°C, cooled down to 25°C at a rate of 0.33°C/min and equilibrated at 25°C for 12 h. CDN Y, including the constituents LDH/NAD+-DD′, LDH-DC′, CD′-NAD+, CC′ was prepared as follows: LDH-D (20 µL, 100 µM), D′-NAD+ (20 µL, 100 µM), C (20 µL, 100 µM), C′ (20 µL, 100 µM) were mixed in Tris buffer (10 mM, pH = 7.29) that includes 20 mM MgCl2 and 100 mM K+. The mixture was annealed at 37°C for 1 h, cooled down to 25°C at a rate of 0.33°C/min, and equilibrated at 25°C for 12 h.
For the triggered transition of CDN X, triggers T1, T1′ or T2, T2′ are 1.67-fold excess than each component of CDN. After adding triggers into the initial CDN, the final concentration of each component of CDN was 1 µM and the final concentration of trigger was 1.67 µM. The solution was incubated at 28°C overnight to equilibrate. For the triggered transition of CDN Y, triggers T3, T3′ or T4, T4′ is 2.5-fold excess than each component of CDN. After adding triggers into the initial CDN, the final concentration of each component of CDN was 1 µM and the final concentration of trigger was 2.5 µM. The solution was incubated at 28°C overnight to equilibrate. After equilibration, the equilibrated CDN (each component 1 µM) was treated with one substrate (5 µM) (sub 1 for AA′, sub 2 for BB′, sub 3 for BA′, sub 4 for AB′, sub 5 for DC′, sub 6 for CD′, sub 7 for CC′, and sub 8 for DD′). The time-dependent fluorescence changes generated by the cleavage of the different substrates by DNAzyme reporter units were measured. By following the rate of formation of the fluorophore-labeled fragment and using appropriate calibration curves of the intact constituent (Supplementary Figs. 4–5 and 9–10), the quantitative evaluation of the concentrations of constituents is achieved.
All the oligonucleotides (including the names and sequences) used in this study were shown in Supplementary Tables 12–15. The base-pairing probabilities were analyzed using an online platform, NUPACK web application (http://www.nupack.org/).
Mass data were collected using Mass Hunter Workstation software 6.00. The data were analyzed using Mass Hunter Quantitative Analysis B.06.00.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
All data are available in the main text or the supplementary materials and can be obtained from the corresponding author upon reasonable request. Source data are provided with this paper.
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Our research is supported by the Israel Science Foundation.
The authors declare no competing interests.
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Wang, C., O’Hagan, M.P., Neumann, E. et al. Integration of photocatalytic and dark-operating catalytic biomimetic transformations through DNA-based constitutional dynamic networks. Nat Commun 12, 4224 (2021). https://doi.org/10.1038/s41467-021-24512-y