Antimicrobial agents targeting peptidoglycan have shown
successful results in eliminating bacteria with high selective
toxicity. Bacteriophage encoded endolysin as an alternative
antibiotics is a peptidoglycan degrading enzyme with a low
rate of resistance. Here, the engineered endolysin was developed
to defeat multiple drug-resistant (MDR) Acinetobacter
baumannii. First, putative endolysin PA90 was predicted by
genome analysis of isolated Pseudomonas phage PBPA. The
His-tagged PA90 was purified from BL21(DE3) pLysS and
tested for the enzymatic activity using Gram-negative pathogens
known for having a high antibiotic resistance rate including
A. baumannii. Since the measured activity of PA90
was low, probably due to the outer membrane, cell-penetrating
peptide (CPP) DS4.3 was introduced at the N-terminus
of PA90 to aid access to its substrate. This engineered endolysin,
DS-PA90, completely killed A. baumannii at 0.25 μM,
at which concentration PA90 could only eliminate less than
one log in CFU/ml. Additionally, DS-PA90 has tolerance to
NaCl, where the ~50% of activity could be maintained in the
presence of 150 mM NaCl, and stable activity was also observed
with changes in pH or temperature. Even MDR A. baumannii
strains were highly susceptible to DS-PA90 treatment:
five out of nine strains were entirely killed and four strains
were reduced by 3–4 log in CFU/ml. Consequently, DS-PA90
could protect waxworm from A. baumannii-induced death
by ~70% for ATCC 17978 or ~44% for MDR strain 1656-2
infection. Collectively, our data suggest that CPP-fused endolysin
can be an effective antibacterial agent against Gramnegative
pathogens regardless of antibiotics resistance mechanisms.
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Bacteriophage therapy was an ascendant technology for combating
bacterial infections before the golden age of antibiotics,
but the therapeutic potential of phages was largely ignored
after the discovery of penicillin. Recently, with antibioticresistant
infections on the rise, these phages are receiving renewed
attention to combat problematic bacterial infections.
Our approach is to enhance bacteriophages with antimicrobial
peptides, short peptides with broad-spectrum antibiotic or
antibiofilm effects. We inserted coding sequences for 1018,
an antimicrobial peptide previously shown to be an effective
broad-spectrum antimicrobial and antibiofilm agent, or the
fluorescent marker mCherry, into the T7Select phage genome.
Transcription and production of 1018 or mCherry began
rapidly after E. coli cultures were infected with genetically modified
phages. mCherry fluorescence, which requires a 90 min
initial maturation period, was observed in infected cultures
after 2 h of infection. Finally, we tested phages expressing 1018
(1018 T7) against bacterial planktonic cultures and biofilms,
and found the 1018 T7 phage was more effective than the
unmodified T7Select phage at both killing planktonic cells and
eradicating established biofilms, validating our phage-driven
antimicrobial peptide expression system. The combination
of narrow-spectrum phages delivering relatively high local
doses of broad-spectrum antimicrobials could be a powerful method to combat resistant infections. The experiments we
describe prove this combination is feasible in vitro, but further
testing and optimization are required before genetically modified
phages are ready for use in vivo.
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