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Mutations in Escherichia coli aceE and ribB Genes Allow Survival of Strains Defective in the First Step of the Isoprenoid Biosynthesis Pathway

  • Jordi Perez-Gil,

    Affiliation Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain

  • Eva Maria Uros,

    Affiliation Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain

  • Susanna Sauret-Güeto,

    Current address: John Innes Centre, Colney, Norwich, United Kingdom

    Affiliation Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain

  • L. Maria Lois,

    Affiliation Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain

  • James Kirby,

    Affiliation Joint BioEnergy Institute, Emeryville, California, United States of America

  • Minobu Nishimoto,

    Affiliation Joint BioEnergy Institute, Emeryville, California, United States of America

  • Edward E. K. Baidoo,

    Affiliation Joint BioEnergy Institute, Emeryville, California, United States of America

  • Jay D. Keasling,

    Affiliation Joint BioEnergy Institute, Emeryville, California, United States of America

  • Albert Boronat,

    Affiliations Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain, Department de Bioquímica i Biologia Molecular, Universitat de Barcelona, Barcelona, Spain

  • Manuel Rodriguez-Concepcion

    Affiliation Centre for Research in Agricultural Genomics (CRAG) CSIC-IRTA-UAB-UB, Campus UAB Bellaterra, Barcelona, Spain


A functional 2-C-methyl-D-erythritol 4-phosphate (MEP) pathway is required for isoprenoid biosynthesis and hence survival in Escherichia coli and most other bacteria. In the first two steps of the pathway, MEP is produced from the central metabolic intermediates pyruvate and glyceraldehyde 3-phosphate via 1-deoxy-D-xylulose 5-phosphate (DXP) by the activity of the enzymes DXP synthase (DXS) and DXP reductoisomerase (DXR). Because the MEP pathway is absent from humans, it was proposed as a promising new target to develop new antibiotics. However, the lethal phenotype caused by the deletion of DXS or DXR was found to be suppressed with a relatively high efficiency by unidentified mutations. Here we report that several mutations in the unrelated genes aceE and ribB rescue growth of DXS-defective mutants because the encoded enzymes allowed the production of sufficient DXP in vivo. Together, this work unveils the diversity of mechanisms that can evolve in bacteria to circumvent a blockage of the first step of the MEP pathway.


Isoprenoids (also called terpenoids) are a ubiquitous and highly diverse family of compounds produced from the five-carbon precursor isopentenyl diphosphate (IPP) and its double-bond isomer dimethylallyl diphosphate (DMAPP) in all living organisms [1][3]. These precursors are synthesized from acetyl-CoA by the mevalonic acid (MVA) pathway in archaea (archaebacteria), fungi, and animals. By contrast, the unrelated 2-C-methyl-D-erythritol 4-phosphate (MEP) pathway produces IPP and DMAPP from pyruvate and glyceraldehyde 3-phosphate in most bacteria (eubacteria) and apicomplexan protozoa, including important human pathogens such as those causing tuberculosis and malaria [3][5]. Because the MEP pathway is essential in such pathogens but is not present in animals, it has been proposed as a promising target for the design of new antibacterial and antimalarial agents that would be potentially innocuous for humans [6][8]. However, we still know little about possible mechanisms of resistance to current and potential drugs targeting the MEP pathway in bacterial pathogens.

The genes and enzymes of the MEP pathway are best characterized in Escherichia coli. The initial reaction of the pathway (Fig. 1) is catalyzed by 1-deoxy-D-xylulose 5-phosphate (DXP) synthase (DXS, encoded by the dxs gene) and involves the condensation of (hydroxyethyl)thiamine, derived from pyruvate, with the C1 aldehyde group of D-glyceraldehyde 3-phosphate to produce DXP [9][11]. In the second step, an intramolecular rearrangement and reduction of DXP by the enzyme DXP reductoisomerase (DXR, encoded by the ispC/yaeE/dxr gene) yields MEP [12], [13]. An alternative oxidoreductase enzyme with a DXR-like (DRL) activity was recently found in a reduced number of bacteria [14]. MEP produced by DXR or DRL is eventually converted to both IPP and DMAPP by sequential activities of the enzymes encoded by the genes ispD/ygbP, ispE/ychB, ispF/ygbP, ispG/gcpE, and ispH/lytB [5], [15].

Figure 1. Biosynthesis of isoprenoid precursors in E. coli.

The indicated genes (in italics) encode enzymes that produce the first intermediates of the MEP pathway either originally (dxs, dxr) or by mutation as indicated by asterisks (aceE, ribB). The E. coli strains used in this work are engineered to synthesize isopentenyl diphosphate (IPP) and dimethylallyl diphosphate (DMAPP) from exogenously supplied mevalonic acid (MVA). GAP, D-glyceraldehyde 3-phosphate; DXP, 1-deoxy-D-xylulose 5-phosphate; MEP, 2-C-methyl-D-erythritol 4-phosphate.

The best studied inhibitor of the MEP pathway is fosmidomycin (FSM), a specific inhibitor of the enzyme DXR which also inhibits DRL [14], [16][19]. The uptake of FSM by bacterial cells is an active process involving a cAMP-dependent glycerol 3-phosphate transporter (GlpT) protein [20]. Loss of GlpT activity in E. coli mutants or the absence of a GlpT homologue in other bacteria such as Mycobacterium tuberculosis or Brucella abortus leads to FSM resistance [14], [20], [21]. Enhanced export of the inhibitor by overexpression of the E. coli fsr gene also results in FSM resistance [22]. Antibiotic resistance can result not only from interfering with drug transport or mode of action but also from the use of an alternative pathway not affected by the inhibitor. To investigate the relevance of the latter type of mechanisms for resistance to MEP pathway inhibitors, we aimed to identify spontaneous mutations that could suppress an otherwise lethal obstruction of the pathway in living bacteria.

Loss of function of the MEP pathway in E. coli can be rescued in strains containing a synthetic MVA operon that allows the production of IPP and DMAPP from exogenously supplied MVA (Fig. 1) [23], [24]. However, in cells harboring a deletion of the dxs gene (strain EcAB4-2), MVA auxotrophy was suppressed with a relatively high frequency (6.4 per 109 cells) by mutations in other genes [25]. As a result, colonies of DXS-defective suppressor mutants could grow overnight on plates lacking MVA. Suppressor mutants were also found in the DXR-deficient strain EcAB4-10, although with a slightly lower frequency (2.4 per 109 cells) and poor growth. No suppressor mutants were found in strains with disruptions to the other MEP pathway genes [25]. These results suggested that bacteria can respond to a block of DXS or DXR activities by using other proteins that deliver DXP or MEP when mutated [25]. In this work we identify genes and mutations that allow survival of DXS-deficient strains and demonstrate that the mutant proteins are indeed able to synthesize DXP (or a precursor molecule) in vivo.

Materials and Methods

Bacterial strains and screening for suppressor mutants

Disruption of individual MEP pathway genes in E. coli strains EcAB4-2 (dxs::CAT) and EcAB4-10 (dxr::CAT), each containing a chromosomal copy of a synthetic MVA operon, was carried out as described [25] by deleting most of their coding region and introducing chloramphenicol resistance (CAT) genes. Similarly, strain EcAB1-6 (dxs::CAT dxr::TET) was constructed by disrupting both dxs and dxr genes with chloramphenicol and tetracycline resistance genes, respectively, in MC4100 cells harboring the MVA operon in plasmid pAB-M3 [23], [26]. For isolation of suppressor mutants, EcAB4-2 cells were cultured at 37°C in Luria broth (LB) medium supplemented with 1 mM MVA, 25 µg/ml kanamycin (to select for the MVA operon) and 17 µg/ml chloramphenicol (to select for the disruption of the dxs gene) until exponential phase. After cells were pelleted and rinsed twice with LB, several batches of ca.108 cells (estimated by measuring optical density at 600 nm, OD600) were plated on LB agar containing only kanamycin and chloramphenicol. In some plates, a paper disk soaked in 30 µl ethylmethane sulphonate (EMS) was placed on the surface of the medium to induce mutations. Spontaneous and EMS-induced mutants that formed a colony in the absence of MVA were analyzed to confirm the deletion of the dxs genes by PCR.

Identification of the genes mutated in the suppressor lines

Genomic DNA from suppressor mutants was isolated as described [25], [27] and partially digested with Sau3A. Fragments of 2–4 kb were gel-purified using the Qiaquick (Qiagen) system and ligated into the BamHI site of pUC19. After amplification of the genomic library in TOP10 cells, EcAB4-2 competent cells were transformed with aliquots of the library, and transformants resistant to kanamycin, chloramphenicol, and 100 µg/ml ampicillin that were able to grow without MVA were selected. Plasmid DNA isolated from these transformants was used to transform new EcAB4-2 cells to confirm that it conferred the ability to grow in the absence of MVA. Positive clones were sequenced to identify the gene (and the mutation) responsible for the suppression phenotype. Screenings for mutations specifically in aceE and ribB were carried out by amplification of their coding regions by colony PCR with high-fidelity AccuPrime DNA polymerase (Invitrogen), followed by sequencing.

Plasmid constructs

The wild-type and mutant aceE and ribB genes (including the promoter region) were amplified from EcAB4-2 and suppressor mutant cells by PCR using AccuPrime DNA polymerase and primers aceE-1F (5′- C C A G A A G A T G T T G T A A A T C A A G C -3′) and aceE-4R (5′- T T T A C C T C T T A C G C C A G A C G -3′) for aceE and ribB-pNF (5′- A G C A T A T G A G T G C C A T T G T A G T G-3′) and ribB-XR (5′- A G T C A C T C G A G G C T G G C T T T A C G C T C A T G T G C-3′) for ribB. The PCR products were gel-purified and cloned into pCRII-TOPO (Invitrogen). Inserts were sequenced using vector and gene-specific primers to confirm the presence of the identified mutations.

Detection of DXP in cell extracts

EcAB1-6 cells were transformed with plasmids harboring wild type and mutant versions of aceE or ribB (or an empty pCRII-TOPO plasmid as a control) and positive transformants were selected on LB plates supplemented with 1 mM MVA, 50 µg/ml kanamycin (to select for the pCRII-TOPO constructs), 100 µg/ml ampicillin (to select for the pAB-M3 plasmid with the MVA operon), 17 µg/ml chloramphenicol (to select for the disruption of the dxs gene), and 5 µg/ml tetracyclin (to select for the disruption of the dxr gene). Individual colonies were then grown at 37°C overnight in liquid media with the same supplements. The overnight cultures were used to confirm the identity of the strain and plasmids by PCR and restriction analysis and to inoculate fresh 10 ml cultures to an OD600 of 0.05. Inoculated cultures were grown at 37°C for 5 hours and aliquots corresponding to an OD600 of 10 were then collected. Cells were pelleted and immediately resuspended in 200 μl of 1∶1 (v/v) methanol: water. Cell suspensions were loaded in Amicon Ultra-0.5 centrifugal filter devices and spun at 14,000 rpm and 4°C for 90 min in a refrigerated microfuge. DXP was detected and quantified in the flow-through by liquid chromatography and mass spectrometry (LC-MS).

LC was conducted on an ZIC-pHILIC column of 150-mm length, 2.1-mm internal diameter, and 5-µm particle size (Merck SeQuant), using an Agilent 1200 Series HPLC system. A sample injection volume of 2 µL was used throughout. The temperature of the sample tray was maintained at 4°C by an Agilent FC/ALS Thermostat. The column compartment was set to 50°C. The mobile phases used were composed of A) 80 mM ammonium carbonate and B) acetonitrile. Isocratic elution was achieved at 68% B via a flow rate of 0.23 mL/min for 12 min. From there the flow rate was gradually increased to 0.3 mL/min until 12.5 min. The flow rate was then held at 0.3 mL/min for a further 2.5 min. The HPLC system was coupled to an Agilent 6210 time-of-flight mass spectrometer (LC-TOF MS), by a 1/3 post-column split. Contact between both instrument set-ups was established by a LAN card in order to trigger the MS into operation upon the initiation of a run cycle from the MassHunter workstation (Agilent). Nitrogen gas was used as both the nebulizing and drying gases to facilitate the production of gas-phase ions. The drying and nebulizing gases were set to 10 L/min and 25 psi, respectively, and a drying gas temperature of 300°C was used throughout. Electrospray ionization (ESI) was conducted in the negative ion mode and a capillary voltage of –3500 V was utilized. MS experiments were carried out in the full scan mode, at 0.86 spectra/ sec and a cycle time of 1.1162.8 sec, for the detection of [M–H]- ions. The instrument was tuned for a range of 50–1700 m/z. Prior to LC-ESI-TOF MS analysis, the TOF MS was calibrated via an ESI-L-low concentration tuning mix (Agilent). Data acquisition and processing were performed by the MassHunter software package. DXP was quantified via a five-point calibration curve. The R2 coefficient for the calibration curve was >0.99. The chemical standard for DXP (Echelon) was made up to 500 µM, as the stock solution, in methanol-water (50∶50, v/v).


Most DXS-defective suppressor mutants harbour mutations in the aceE gene

To investigate the mechanisms by which bacteria could survive in the absence of a DXS enzyme, we aimed to identify the genes responsible in a collection of DXS-defective suppressor mutants (SX lines). Previous screening for suppressors of MVA auxotrophy in DXS-defective EcAB4-2 cells (i.e. the lethality caused by dxs deletion) resulted in the isolation of 6 spontaneous mutants (SX1 to SX6) [25]. A second screening led to the isolation of 14 more spontaneous mutants (SX7 to SX20) and 14 EMS-induced mutants (SX1E to SX14E). However, 6 spontaneous mutants and 2 EMS-induced mutants lost the ability to grow without MVA after storage as glycerol stocks and re-streaking on fresh LB plates supplemented only with kanamycin and ampicillin. Of the remaining 26 mutants, one (SX5) was previously reported to harbor a missense mutation in the aceE gene (encoding the catalytic E1 subunit of the pyruvate dehydrogenase complex, PDH), resulting in an E636Q change in the protein sequence [25]. Sequencing of the aceE gene in the remaining mutants identified a total of 4 different mutations (Table 1). In particular, the E636Q mutation was found in 2 other strains besides SX5, whereas 1 clone had a different mutation in the same residue (E636G). Two more aceE mutations were found: Q408R in 1 strain and L633R in 17 clones. In total, 22 out of 26 suppressor SX mutants contained mutations in the aceE gene, suggesting that the alteration of PDH activity might be the most common mechanism of resistance to the inhibition of DXS activity.

Table 1. Ocurrence of identified mutations in EcAB4-2 cells.

A mutant ribB gene was found in the remainder of the DXS-deficient suppressors

To identify the genetic change responsible for the bypass of DXS activity in the 4 remaining strains with no mutations in aceE (SX6, SX7, SX18, and SX12E), we followed a strategy similar to that previously described for SX5 [25]. We selected strain SX18 to construct a genomic library in pUC19. After amplification, DXS-defective EcAB4-2 cells were transformed with the library, and colonies able to grow without MVA were selected to isolate the incorporated plasmid and sequence the corresponding inserts. All the isolated plasmids were found to contain a mutation in the ribB gene, encoding 3,4-dihydroxy-2-butanone 4-phosphate synthase (DHBPS). This enzyme catalyzes the conversion of D-ribulose 5-phosphate to formate and 3,4-dihydroxy-2-butanone 4-phosphate, the latter serving as the biosynthetic precursor for the xylene ring of riboflavin [28]. Complete sequencing of the ribB gene in strains SX6, SX7 and SX12E also found mutations in this gene. In particular, a missense mutation resulting in a G108S change in DHBPS was found in SX18 and SX12E, whereas clones SX6 and SX7 harbored a D113G change (Table 1).

The identified mutations are sufficient to rescue the loss of DXS activity in EcAB4-2 cells

To confirm whether the new mutations identified in aceE and ribB were actually responsible for the suppression phenotype, wild type and mutant versions of these genes (including their promoters) were amplified from the parental EcAB4-2 strain and the corresponding suppressor mutants, respectively, and used to complement EcAB4-2 cells. As shown previously [25], the plasmid carrying the E636Q mutation in aceE rescued growth on plates without MVA, whereas the wild type gene did not complement the loss of DXS activity in EcAB4-2 (Fig. 2). The other aceE mutations (Q408R, L633R, and E636G) were also able to rescue MVA auxotrophy of the strain. Similarly, the two identified mutant forms of ribB (G108S and D113G), but not the wild type version, rescued growth of DXS-defective EcAB4-2 cells in medium without MVA (Fig. 2). These results suggest that the presence of any of the identified mutations in aceE or ribB results in altered enzymes (PDH or DHBPS, respectively) that each produce a metabolite that can ultimately be converted to isoprenoids in the absence of a functional DXS activity.

Figure 2. Complementation of E.coli strains defective in DXS or DXR.

Cells were transformed with pCRII-TOPO constructs and plated on LB medium containing chloramphenicol (for the disruption of chromosomal dxs or dxr genes), kanamycin (for the MVA operon) and ampicillin (for the introduced plasmid). The medium was supplemented (+) or not (−) with MVA as indicated. Plates were incubated at 37°C for 20 h. (A) Position of transformants harboring plasmids with the indicated wild type or mutant (asterisks) genes or an empty vector control (Ø). (B) EcAB4-2 (dxs::CAT) transformants. (C) EcAB4-10 (dxr::CAT) transformants.

Mutant aceE and ribB genes allow the production of DXP in vivo

The bypass of DXS by mutant forms of PDH and DHBPS enzymes might result either from the production of DXP or an alternative substrate for DXR, or from the supply of MEP or a downstream metabolite of the pathway (Fig. 1). The latter possibility can be addressed by using a genetic strategy based on the complementation of the DXR-deficient strain EcAB4-10. Thus, the putative production of MEP or a downstream MEP pathway intermediate by the mutant enzymes would allow not only DXS-defective but also DXR-defective cells to grow in the absence of MVA (Fig. 1). However, when EcAB4-10 cells were transformed with the constructs containing mutant aceE and ribB genes, transformants could only be recovered on MVA-containing plates because none of them were able to rescue MVA auxotrophy (Fig. 2). These results confirm that the mutant PDH and DHBPS enzymes synthesize a product that enters the MEP pathway upstream of the reaction catalyzed by DXR.

To discriminate between the remaining possibilities (i.e. the mutant enzymes allow the production of either DXP or another metabolite that can be used as an alternative substrate for DXR), we investigated whether the presence of mutant versions of PDH or DHBPS resulted in the production of DXP in cells lacking both DXS and DXR activities (strain EcAB1-6). After transformation of the EcAB1-6 strain with plasmids containing wild type and mutant versions of both aceE and ribB, cells were grown in MVA-supplemented liquid medium and harvested in the exponential growth phase. HPLC-MS/MS analysis of cell extracts from controls transformed with an empty plasmid showed the presence of low but detectable levels of DXP (Fig. 3), indicating that E. coli cells devoid of DXS activity can still produce trace amounts of this metabolite. Levels of DXP in transformants carrying plasmids with wild type versions of aceE or ribB genes were similar to those in the negative control. By contrast, strains expressing the mutant genes showed ca. 20-fold higher DXP levels (Fig. 3), confirming that the corresponding mutant enzymes are able to synthesize DXP (or a metabolite that can be transformed into DXP by the cells) in vivo.

Figure 3. DXP levels in cells expressing wild type and mutant aceE and ribB genes.

E.coli cells defective in both DXS and DXR were transformed with pCRII-TOPO constructs with the indicated wild type or mutant genes or an empty vector control (Ø). Positive transformants were grown in triplicate for 5 h with MVA, and DXP levels were measured by LC-MS. Mean and standard deviation (n = 3) values are represented relative to the levels in Ø controls.


In bacteria, isoprenoids play essential roles in a variety of processes that are vital for growth and survival, including cell wall and membrane biosynthesis, electron transport, and conversion of light into chemical energy [29]. Also, many microorganisms produce isoprenoid secondary metabolites of economic relevance [30]. Since the discovery of the MEP pathway in the mid 1990 s, it became more and more evident that bacteria display a wide metabolic plasticity regarding the route to produce isoprenoids. Most bacteria only use the MEP pathway for IPP and DMAPP biosynthesis, but there are exceptions to this trend. Some bacteria synthesize their isoprenoid precursors using the MVA pathway instead of the MEP pathway, whereas there are parasitic bacteria that lack both pathways (likely because they obtain their isoprenoids from host cells) and also organisms that possess the two full pathways [3], [31][34]. Most strikingly, related bacteria may use different pathways for isoprenoid biosynthesis while unrelated bacteria may use the same pathway. In addition to the MEP and MVA pathways, alternative pathways and metabolic intermediates have been proposed for isoprenoid biosynthesis in the cyanobacterium Synechocystis PCC 6803, which lacks the MVA pathway and does not appear to use the canonical MEP pathway under photosynthetic conditions [35], [36]. Diversity can be found also at the level of individual pathway steps, with several examples of reactions catalyzed by different classes of enzymes with no sequence, structural, or catalytic similarity [14], [17], [33], [37]. In at least some cases, it is clear that the alternative routes to MEP pathway intermediates resulted from the recruitment of available enzymes that were not related to isoprenoid synthesis. But we still know very little about the genes and enzymes that could potentially contribute to isoprenoid biosynthesis, despite the relevance of this knowledge to both development of efficient antibiotics and metabolic engineering of isoprenoid biosynthesis. Here we show that the MEP pathway intermediate DXP can be produced (although at very low levels) in the absence of a functional DXS-encoding gene, suggesting that other enzymes might produce this metabolite, perhaps as a by-product. However, such trace levels are not sufficient to support bacterial growth and survival. We also provide biochemical and genetic evidence of novel routes for efficient DXP synthesis arising from specific mutations in two E. coli genes, aceE and ribB (encoding PDH and DHBPS, respectively).

The E636Q mutation in PDH was previously shown to rescue the deficiency of DXS but not DXR activity in vivo [25]. In this work, we have identified three more mutations (Q408R, L633R, and E636G) that allow PDH to catalyze an unknown reaction that eventually results in the production of DXP in the absence of endogenous DXS activity. Like DXS, PDH is a thiamine diphosphate (TPP) dependent carboligase that catalyzes the decarboxylation of pyruvate with the formation of hydroxyethyl-TPP as an intermediate. In fact, purified PDH has been shown to catalyze the formation of 1-deoxy-D-xylulose (DX) from pyruvate and D-glyceraldehyde [38], [39]. DX can be phosphorylated to DXP by the kinase encoded by the xylB gene in E. coli [40]. However, our results suggest that in vivo the wild type PDH enzyme does not produce enough DX (or DXP, using D-glyceraldehyde 3-phosphate) to rescue the loss of DXS activity since only the mutant enzyme is able to complement the dxs knockout (Fig. 2) and to cause an accumulation of DXP beyond background levels (Fig. 3).

In the case of DHBPS, the proposed mechanism for the conversion of D-ribulose 5-phosphate to formate and 3,4-dihydroxy-2-butanone 4-phosphate involves a complex series of steps including dehydration, intramolecular rearrangement and rehydration [41]. Interestingly, the alternative route into the MEP pathway proposed in Synechocystis PCC 6803 appears to be stimulated by D-xylulose 5-phosphate and also by dihydroxyacetone phosphate [35], [36]. We therefore speculate that either D-ribulose 5-phosphate or its isomer D-xylulose 5-phospate might be converted to DXP by mutant G108S or D113G enzymes. We intend to further investigate the metabolic route to the DXP pathway enabled by mutant DHBPS enzymes using these and alternative substrates and considering the option that a metabolite may be generated that serves as an intermediate for DXP synthesis.

In summary, our work demonstrates that bacteria can circumvent a blockage of the MEP pathway at the level of DXS by mutation of either of two genes (aceE and ribB). Based on these results, DXS is not a good target for the development of new antibiotics, since resistance is likely to be developed very easily. On the other hand, DXP production appears to be one of the main flux-determining steps of the MEP pathway because overexpression of DXS-encoding genes has been shown to result in an enhanced production of MEP-derived isoprenoids in bacteria and plants [30], [42]. We are currently investigating whether the use of mutant PDH and DHBPS enzymes could be a good strategy to overproduce DXP in metabolic engineering approaches.


We thank Anna Orozco and Rosa Rodriguez for valuable technical assistance.

Author Contributions

Conceived and designed the experiments: JPG EMU SSG JK JDK AB MRC. Performed the experiments: JPG EMU SSG JK MN EEKB MRC. Analyzed the data: JPG EMU SSG JK MN EEKB JDK AB MRC. Contributed reagents/materials/analysis tools: JPG EMU SSG LML JK MN EEKB. Wrote the paper: MRC.


  1. 1. Bouvier F, Rahier A, Camara B (2005) Biogenesis, molecular regulation and function of plant isoprenoids. Prog Lipid Res 44: 357–429.
  2. 2. Sacchettini JC, Poulter CD (1997) Creating isoprenoid diversity. Science 277: 1788–1789.
  3. 3. Hemmerlin A, Harwood JL, Bach TJ (2012) A raison d'etre for two distinct pathways in the early steps of plant isoprenoid biosynthesis? Prog Lipid Res 51: 95–148.
  4. 4. Lichtenthaler HK, Rohmer M, Schwender J (1997) Two independent biochemical pathways for isopentenyl diphosphate and isoprenoid biosynthesis in higher plants. Physiologia plantarum 101: 643–652.
  5. 5. Rodríguez-Concepción M, Boronat A (2002) Elucidation of the methylerythritol phosphate pathway for isoprenoid biosynthesis in bacteria and plastids. A metabolic milestone achieved through genomics. Plant Physiol 130: 1079–1089.
  6. 6. Rohdich F, Bacher A, Eisenreich W (2005) Isoprenoid biosynthetic pathways as anti-infective drug targets. Biochem Soc Trans 33: 785–791.
  7. 7. Rodriguez-Concepcion M (2004) The MEP pathway: a new target for the development of herbicides, antibiotics and antimalarial drugs. Curr Pharm Des 10: 2391–2400.
  8. 8. Davey MS, Tyrrell JM, Howe RA, Walsh TR, Moser B, et al. (2011) A promising target for treatment of multidrug-resistant bacterial infections. Antimicrob Agents Chemother 55: 3635–3636.
  9. 9. Lois LM, Campos N, Putra SR, Danielsen K, Rohmer M, et al. (1998) Cloning and characterization of a gene from Escherichia coli encoding a transketolase-like enzyme that catalyzes the synthesis of D-1-deoxyxylulose 5-phosphate, a common precursor for isoprenoid, thiamin, and pyridoxol biosynthesis. Proc Natl Acad Sci USA 95: 2105–2110.
  10. 10. Sprenger GA, Schorken U, Wiegert T, Grolle S, de Graaf AA, et al. (1997) Identification of a thiamin-dependent synthase in Escherichia coli required for the formation of the 1-deoxy-D-xylulose 5-phosphate precursor to isoprenoids, thiamin, and pyridoxol. Proc Natl Acad Sci USA 94: 12857–12862.
  11. 11. Lange BM, Wildung MR, McCaskill D, Croteau R (1998) A family of transketolases that directs isoprenoid biosynthesis via a mevalonate-independent pathway. Proc Natl Acad Sci USA 95: 2100–2104.
  12. 12. Kuzuyama T, Takahashi S, Watanabe H, Seto H (1998) Direct formation of 2-C-methyl-D-erythritol 4-phosphate from 1-deoxy-D-xylulose 5-phosphate by 1-deoxy-D-xylulose 5-phosphate reductoisomerase, a new enzyme in the non-mevalonate pathway to isopentenyl diphosphate. Tetrahedron Letters 39: 4509–4512.
  13. 13. Takahashi S, Kuzuyama T, Watanabe H, Seto H (1998) A 1-deoxy-D-xylulose 5-phosphate reductoisomerase catalyzing the formation of 2-C-methyl-D-erythritol 4-phosphate in an alternative non-mevalonate pathway for terpenoid biosynthesis. Proc Natl Acad Sci USA 95: 9879–9884.
  14. 14. Sangari FJ, Perez-Gil J, Carretero-Paulet L, Garcia-Lobo JM, Rodriguez-Concepcion M (2010) A new family of enzymes catalyzing the first committed step of the methylerythritol 4-phosphate (MEP) pathway for isoprenoid biosynthesis in bacteria. Proc Natl Acad Sci U S A 107: 14081–14086.
  15. 15. Hunter WN (2007) The non-mevalonate pathway of isoprenoid precursor biosynthesis. J Biol Chem 282: 21573–21577.
  16. 16. Steinbacher S, Kaiser J, Eisenreich W, Huber R, Bacher A, et al. (2003) Structural basis of fosmidomycin action revealed by the complex with 2-C-methyl-D-erythritol 4-phosphate synthase (IspC). Implications for the catalytic mechanism and anti-malaria drug development. J Biol Chem 278: 18401–18407.
  17. 17. Perez-Gil J, Calisto BM, C B, Kurz T, Fita I, et al. (2012) Crystal structure of the Brucella abortus deoxyxylulose 5-phosphate reductoisomerase-like (DRL) enzyme involved in isoprenoid biosynthesis. J Biol Chem 287: 15803–15809.
  18. 18. Kuzuyama T, Shimizu T, Takahashi S, Seto H (1998) Fosmidomycin, a specific inhibitor of 1-deoxy-D-xylulose 5-phosphate reductoisomerase in the nonmevalonate pathway for terpenoid biosynthesis. Tetrahedron Letters 39: 7913–7916.
  19. 19. Zeidler J, Schwender J, Muller C, Wiesner J, Weidemeyer C, et al. (1998) Inhibition of the non-mevalonate 1-deoxy-D-xylulose-5-phosphate pathway of plant isoprenoid biosynthesis by fosmidomycin. Z Naturfosch 53c: 980–986.
  20. 20. Sakamoto Y, Furukawa S, Ogihara H, Yamasaki M (2003) Fosmidomycin resistance in adenylate cyclase deficient (cya) mutants of Escherichia coli. Biosci Biotechnol Biochem 67: 2030–2033.
  21. 21. Brown AC, Parish T (2008) Dxr is essential in Mycobacterium tuberculosis and fosmidomycin resistance is due to a lack of uptake. BMC Microbiol 8: 78.
  22. 22. Fujisaki S, Ohnuma S, Horiuchi T, Takahashi I, Tsukui S, et al. (1996) Cloning of a gene from Escherichia coli that confers resistance to fosmidomycin as a consequence of amplification. Gene 175: 83–87.
  23. 23. Campos N, Rodriguez-Concepcion M, Sauret-Gueto S, Gallego F, Lois LM, et al. (2001) Escherichia coli engineered to synthesize isopentenyl diphosphate and dimethylallyl diphosphate from mevalonate: a novel system for the genetic analysis of the 2-C-methyl-D-erythritol 4-phosphate pathway for isoprenoid biosynthesis. Biochem J 353: 59–67.
  24. 24. Kakinuma K, Dekishima Y, Matsushima Y, Eguchi T, Misawa N, et al. (2001) New approach to multiply deuterated isoprenoids using triply engineered Escherichia coli and its potential as a tool for mechanistic enzymology. J Am Chem Soc 123: 1238–1239.
  25. 25. Sauret-Güeto S, Uros EM, Ibanez E, Boronat A, Rodriguez-Concepcion M (2006) A mutant pyruvate dehydrogenase E1 subunit allows survival of Escherichia coli strains defective in 1-deoxy-D-xylulose 5-phosphate synthase. FEBS Lett 580: 736–740.
  26. 26. Rodríguez-Concepción M, Campos N, Maria Lois L, Maldonado C, Hoeffler JF, et al. (2000) Genetic evidence of branching in the isoprenoid pathway for the production of isopentenyl diphosphate and dimethylallyl diphosphate in Escherichia coli. FEBS Lett 473: 328–332.
  27. 27. Pitcher DG, Saunders NA, Owen RJ (1989) Rapid extraction of bacterial genomic DNA with guanidium thiocyanate. Lett Appl Microbiol 8: 151–156.
  28. 28. Richter G, Krieger C, Volk R, Kis K, Ritz H, et al. (1997) Biosynthesis of riboflavin: 3,4-dihydroxy-2-butanone-4-phosphate synthase. Methods Enzymol 280: 374–382.
  29. 29. Rodríguez-Concepción M, Boronat A (2012) Isoprenoid biosynthesis in prokaryotic organisms. In: Bach T, Rohmer M, Gershenzon J, editors. Isoprenoid Synthesis in Plants and Microorganisms. New York: Springer.
  30. 30. Kirby J, Keasling JD (2008) Metabolic engineering of microorganisms for isoprenoid production. Nat Prod Rep 25: 656–661.
  31. 31. Lange BM, Rujan T, Martin W, Croteau R (2000) Isoprenoid biosynthesis: the evolution of two ancient and distinct pathways across genomes. Proc Natl Acad Sci U S A 97: 13172–13177.
  32. 32. Boucher Y, Doolittle WF (2000) The role of lateral gene transfer in the evolution of isoprenoid biosynthesis pathways. Mol Microbiol 37: 703–716.
  33. 33. Laupitz R, Hecht S, Amslinger S, Zepeck F, Kaiser J, et al. (2004) Biochemical characterization of Bacillus subtilis type II isopentenyl diphosphate isomerase, and phylogenetic distribution of isoprenoid biosynthesis pathways. Eur J Biochem 271: 2658–2669.
  34. 34. Kuzuyama T, Seto H (2003) Diversity of the biosynthesis of the isoprene units. Nat Prod Rep 20: 171–183.
  35. 35. Poliquin K, Ershov YV, Cunningham FX Jr, Woreta TT, Gantt RR, et al. (2004) Inactivation of sll1556 in Synechocystis strain PCC 6803 impairs isoprenoid biosynthesis from pentose phosphate cycle substrates in vitro. J Bacteriol 186: 4685–4693.
  36. 36. Ershov YV, Gantt RR, Cunningham Jr FX Jr, Gantt E (2002) Isoprenoid biosynthesis in Synechocystis sp. strain PCC6803 is stimulated by compounds of the pentose phosphate cycle but not by pyruvate or deoxyxylulose-5-phosphate. J Bacteriol 184: 5045–5051.
  37. 37. Kaneda K, Kuzuyama T, Takagi M, Hayakawa Y, Seto H (2001) An unusual isopentenyl diphosphate isomerase found in the mevalonate pathway gene cluster from Streptomyces sp. strain CL190. Proc Natl Acad Sci U S A 98: 932–937.
  38. 38. Schoerken U, Sprenger GA (1998) Thiamin-dependent enzymes as catalysts in chemoenzymatic syntheses. Biochim Biophys Acta 1385(2): 229–243.
  39. 39. Yokota A, Sasajima KI (1986) Formation of 1-deoxyketoses by pyruvate dehydrogenase and acetoin dehydrogenase. Agric Biol Chem 50: 2517–2524.
  40. 40. Wungsintaweekul J, Herz S, Hecht S, Eisenreich W, Feicht R, et al. (2001) Phosphorylation of 1-deoxy-D-xylulose by D-xylulokinase of Escherichia coli. Eur J Biochem 268: 310–316.
  41. 41. Bacher A, Eberhardt S, Fisher M, Kis K, Richter G (2000) Biosynthesis of vitamin B2 (riboflavin). Annu Rev Nutr 20: 153–167.
  42. 42. Rodríguez-Concepción M (2006) Early steps in isoprenoid biosynthesis: Multilevel regulation of the supply of common precursors in plant cells. Phytochem Rev 5: 1–15.